THE EFFECT OF INDOLE-3-CARBINOL AND 3,3’-DIINDOLYLMETHANE ON FATTY ACID SYNTHASE AND SP1 IN BREAST CANCER CELLS
by
George Eramiah Saati
A thesis submitted in conformity with the requirements for the degree of Master of Science Graduate Department of Nutritional Sciences University of Toronto
© Copyright by George Eramiah Saati 2009
THE EFFECT OF INDOLE-3-CARBINOL AND 3,3’-DIINDOLYLMETHANE ON FATTY ACID SYNTHASE AND SP1 IN BREAST CANCER CELLS
Master of Science, 2009 George Eramiah Saati Graduate Department of Nutritional Sciences University of Toronto
ABSTRACT
Fatty acid synthase (FAS), an enzyme that is over-expressed in many cancers, is
necessary for cancer cell proliferation. Previously, we have shown that FAS in cancer cells is
regulated at least in part, by Sp1. Indole-3-carbinol (I3C) and its acid condensation product, 3,3’-
diindolylmethane (DIM) modulate various transcription factors involved in regulating cellular
proliferation and apoptosis. The objective of this study was to determine whether reductions in
breast cancer cell proliferation caused by I3C and/or DIM occur as a result of reductions in FAS.
DIM and, in some cases, I3C reduced FAS expression in three breast cancer cell lines. However,
addition of palmitate or oleate to DIM-treated MCF-7 cells did not restore proliferation. DIM- associated reduction in proliferation of MCF-7 cells also results in a reduction of Sp1 expression, and down-regulation of FAS occurs after inhibition of proliferation. Thus, the anti-proliferative effect of I3C and DIM may be due to their effect on down-regulating Sp1, which in turn could modify several Sp1-associated genes, including FAS.
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ACKNOWLEDGEMENTS
There are a number of special people who were instrumental in making my graduate
experience, one of great enlightenment, excitement and accomplishment. I would like to extend
my sincere gratitude to them here.
First, I would like to thank my supervisor Dr. Michael Archer. Over the past two years,
Dr Archer has shared with me a wealth of knowledge, and given me the encouragement I’ve
needed to successfully complete this degree. He is a true gentleman and everyday around him has truly felt like a privilege. The ways he approaches situations in science and life are some of the most rewarding experiences I’ve ever received. Dr. Archer has helped me mature as an academic and a person. I will take what I have learned from him and do my best to apply as
much of it as I can to my life, in hopes that someday I too can lead myself, my family or an
organization to success – like him.
I would also like to thank my committee members, Dr. Ahmed El-Sohemy and Dr.
Richard Bazinet. I feel very privileged to have met these gentlemen and believe they both will
change the way our world understands nutrition. Dr. El-Sohemy, as one of my committee
members, I am sincerely grateful for your help and advice in completing my thesis work and
experiments. I also would like to thank you for introducing me to the world of nutritional
sciences and research, and for granting me the reference letters and referrals that made it into the
hands of Dr. Archer. Without your help, I don’t know if I would have made it this far
academically. Dr. Bazinet, I am extremely honoured to have had the opportunity to have had you
on my committee. Your unparalleled wisdom, expertise and support were paramount in the
progress and completion of this project. I thank you whole-heartedly for your all your help and suggestions.
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I will always be grateful to the people of Archer lab, whose help has been invaluable in all the years that I have worked in their lab. I would like to thank Suying Lu, Kafi Ealey,
Guodong Liu, Dominic Lau and Wanli Xuan for all their helpful advice and technical assistance.
I am grateful for their friendship and for making my laboratory experience an enjoyable one.
I also want to thank my external examiner, Dr. Wendy Ward, and my examination chair,
Dr. Hanley for being very accommodating and for offering helpful feedback and comments.
Next, I’d like to thank the many graduate students and friends who have made my stay here memorable. To Jennifer Truan, Amin Esfahani, Pedro Huot, Sandra Sacco, Alireza
Jahanmihan, Dennis Wagner, Jovanna Kaludjerovic, Sandra Reza-Lopez, Josh Green, Amanda
Carleton and Julie Mason, I will always be grateful for meeting you. The coffee breaks, the pubs, the restaurants downtown and, of course, the troubleshooting of experiments – I’m very thankful for being able to have shared these experiences with you.
Lastly, I would like to express my utmost love and gratitude to my family. My mother and father have given me an enormous amount of help and understanding and have provided me with food and shelter every single day. Also, my brother and my sister have always been there to lighten my day when I get home. Thank you all for putting up with me during my ups and downs. My family’s continued love and support over the years have helped me become who I am today, and for that, I will be forever grateful.
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TABLE OF CONTENTS
CHAPTER ONE: INTRODUCTION AND LITERATURE REVIEW…………………...….1
Introduction To Diet and Cancer………………………………………………………………….2 Introduction To Thesis…………………………………………………………………………….4
1.1 Cruciferous Vegetables………………………………………………………………………..4 1.1.1 Glucosinolates……………………………………………………………………………….5 1.1.2 Activation of Glucosinolates by Myrosinase………………………………………………..8 1.1.3 Factors Influencing Myrosinase Activity…………………………………………………....9 1.1.4 Bioactive Glucosinolate Products………………………………………………………….11
1.2 Indole-3-Carbinol (I3C) and 3,3'-Diindolylmethane (DIM)…………………………………11 1.2.1 Tissue Distribution, Intake Levels and Physiologic Concentrations………………………12 1.2.2 Cancer Protective Effects of I3C and DIM in Rodents ……………………………………13 1.2.3 Cancer Protective Effects of I3C and DIM in Humans……………………………………17 1.2.4 Anticancer Effects of I3C and DIM in vitro: Possible Mechanisms of Action ……………17
1.3 Fatty Acid Synthesis…………………………………………………………………………22 1.3.1 Fatty Acid Synthase (FAS) and de novo Generation of Palmitate…………………………23 1.3.2 FAS in Normal Tissues…………………………………………………………………….26 1.3.3 Inhibitors of FAS…………………………………………………………………………..27 1.3.4 Regulation of FAS…………………………………………………………………………30 1.3.4.1 Short-term Regulation of FAS…………………………………………………………...30 1.3.4.2 Long-term Regulation of FAS…………………………………………………………...31 1.3.5 Transcription of FAS………………………………………………………………………32
1.4 FAS and Cancer……………………………………………………………………………...35 1.4.1 FAS and Breast Cancer ……………………………………………………………………36 1.4.2 FAS and Other Cancers……………………………………………………………………38 1.4.3 Regulation of FAS in Cancer………………………………………………………………38 1.4.4 Transcription Factors Regulating FAS…………………………………………………….40 1.4.5 Specificity Protein 1 (Sp1) in Cancer…………...…………………………………………42
1.5 Research Hypothesis and Objectives………………………………………………………...44
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CHAPTER TWO: MATERIALS AND METHODS…………………………………………46
2.1 Cell Culture Conditions……………………………………………………………………...47 2.2 Cell Treatment……………………………………………………………………………….47 2.3 Cell Viability Analysis……………………………………………………………………….48 2.4 Preparation of Whole Cell Extracts and Western Blot Analysis……………………………..48 2.5 Preparation of Total RNA……………………………………………………………………49 2.6 Preparation of cDNA and Real-time PCR Analysis………………………………………….50 2.7 Rescue Experiments………………………………………………………………………….51 2.8 Inhibition of FAS with Cerulenin……………………………………………………………52 2.8 Statistical Analysis…………………………………………………………………………...52
CHAPTER THREE: RESULTS……………………………………………………………….53
3.1 The Effect of I3C on MCF-7 Cells…………………………………………………………..54 3.2 The Effect of DIM on MCF-7 Cells………………………………………………………….56 3.3 The Effect of I3C and DIM on MDA-MB-231 Cells………………………………………..59 3.4 The Effect of I3C and DIM on SKBR-3 Cells……………………………………………….61 3.5 MCF-7 Proliferation Restoration Experiments………………………………………………61 3.6 The Effect of DIM on MCF-10A Cells………………………………………………………64 3.7 The Effect of Cerulenin on MCF-10A Proliferation…………………………………………66
CHAPTER FOUR: GENERAL DISCUSSION AND CONCLUSION……………………...68
4.1 Discussion……………………………………………………………………………………69 4.2 Conclusion…………………………………………………………………………………...77 4.3 Implications………………..………………………………………………………………...77 4.4 Limitations and Future Directions..………………………………………………………….78
REFERENCES…………………………………………………………………………………81
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LIST OF TABLES
Table 1.1 - Food sources of selected glucosinolates and their hydrolysis products that are currently under investigation for their cancer chemopreventative properties…………………….7
Table 4.1 – The effect of I3C on proliferation, FAS and Sp1 expression in MCF-7, MDA-MB- 231 and SKBr-3 cells……………………………………………………………….……………70 Table 4.2 – The effect of DIM on proliferation, FAS and Sp1 expression in MCF-7, MDA-MB- 231, SKBr-3 and MCF-10A cells………………………………………….…………………….70
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LIST OF FIGURES
Figure 1.1 - General chemical structure of a glucosinolate molecule…………………………….5
Figure 1.2 - Bioactivation of glucosinolates……………………………………………………...9
Figure 1.3 - Molecular structures of I3C and DIM……………...…………………………...….12
Figure 1.4 – Glycolysis and fatty acid synthesis………………………………………………...23
Figure 1.5 - Palmitate synthesis in FAS enzyme complex……………………………………...25
Figure 1.6 - The FAS promoter region and transcription factor binding areas………………….32
Figure 1.7 - Regulation of FAS expression in cancer by growth factors and steroid hormones…….……………………………………………………………………...39
Figure 1.8 - Post-translational regulation of FAS in cancer by USP2a…………………………40
Figure 3.1 - The effect of I3C on MCF-7 proliferation after 48 h and 72 h…………………….55
Figure 3.2 - The effect of I3C on FAS expression in MCF-7 cells……………………………...55
Figure 3.3 - The effect of DIM on MCF-7 proliferation and FAS expression………………….57
Figure 3.4 - 48h time-course evaluation of DIM on MCF-7 cells……………………………...58
Figure 3.5 – The effect of I3C and DIM on MDA-MB-231cells……………………………….60
Figure 3.6 – The effect of I3C and DIM on SKBR-3 cells…………………………………...... 62
Figure 3.7 - Rescue of DIM-treated MCF-7 Cells with palmitate and oleate…………………..63
Figure 3.8 - The effect of DIM on MCF-10A…………………………………………………..65
Figure 3.9 - The effect of cerulenin on MCF-7 and MCF-10A proliferation………..………….67
Figure 4.1 - I3C/DIM modulates nuclear transcription factor Sp1 and several cancer genes...... 76
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LIST OF ABBREVIATIONS
ACC acetyl-CoA carboxylase ACL ATP-citrate lyase APC adenomatous polyposis coli AhR aryl hydrocarbon receptor AOM azoxymethane ATP adenosine triphosphate BRCA1/2 breast cancer susceptibility protein 1 or 2 cAMP cyclic AMP cAPK cAMP-dependent protein kinase CDK cyclin dependent kinase ChRE carbohydrate response element CIN cervical intraepithelial neoplasia CLA conjugated linoleic acid CPT-1 carnitine palmitoyltransferase-1 CRE cAMP response element CYP cytochrome P450 enzyme DDS dextran sodium sulfate DH β –hydroxyacyl-ACP dehydrase DIM 3,3’-diindolylmethane DMBA 7,12-dimethylbenz (a)-anthracene EGCG epigallocatechin-3-gallate EGF epidermal growth factor EGFR epidermal growth factor receptor ER estrogen receptor ERD enoyl-ACP reductase ERK1/2 extracellular signal-regulated kinase 1 or 2 FAS fatty acid synthase FASKOL FAS knock out in liver GF growth factor GFR growth factor receptor GS glucosinolate HsTL hormone sensitive triacylglycerol lipase I3C indole-3-carbinol IRE insulin response element KS β-ketoacyl synthase KR β-ketoacyl-ACP reductase MAPK mitogen-activated protein kinase MAT malonyl-CoA-ACP transferase MNU methylnitrosourea NFκB nuclear factor κB NNK 4-(methylnitrosamino)-1-(3-pyridyl)-1-butanone
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PEITC phenethyl isothiocynate PhIP 2-amino-1methyl-6-phenylimidazo[4,5-b]pyridine PI3 phosphoinositide-3-kinase SFN sulforaphane SH steroid hormone SHR steroid hormone receptor Sp1 specificity protein 1 SRE sterol response element SREBP sterol regulatory binding protein TE palmitoyl thioesterase TRAMP transgenic adenocarcinoma of the mouse prostate USF upstream stimulatory factor USP2a ubiquitin-specific protease 2a VIN vulval intraepithelial neoplasia XRE xenobiotic response element
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CHAPTER ONE:
INTRODUCTION AND LITERATURE REVIEW
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Introduction to Diet and Breast Cancer
Breast cancer is the most frequent malignancy occurring in women worldwide, and the
second leading cause of cancer death in Canadian women [1]. Globally, incidence and mortality
rates of breast cancer vary dramatically, with industrialized countries, excluding Japan, having
the highest incidence. Amongst industrialized populations, North Americans have the highest
incidence of breast cancer, with rates that are approximately three times higher than the Japanese
[2].
Inheritance of high penetrance susceptibility genes, such as BRCA1 and BRCA2, account for approximately 5% of breast cancer cases, whereas the factors responsible for the remaining
95% remain unclear. However, many epidemiological studies, particularly studies that followed
migrants from lower risk to higher risk countries, have provided strong evidence that diet and
environment play significant roles in the etiology of breast cancer. For example, data from 1962-
1971 on Italians living in Australia showed that while the breast cancer-associated mortality rate in recently arrived Italian migrants was low, it had risen to match that of the Australian-born
population in immigrants that resided there for 17 years or more [3]. Ziegler et al [4] showed that
in females of Chinese, Japanese or Filipino origin who had migrated to the US, breast cancer risk
had increased by as much as 80% in those who resided there for greater than 10 years. Similarly,
Shimizu et al [5] have shown that breast cancer incidence rates in US-born Japanese females is
2.6-fold higher than for Japanese women living in Japan and that, for ‘early-in-life’ Japanese
migrants to the USA, the incidence is 2.4-fold higher. Furthermore, Kolonel et al [6] have shown breast cancer incidence increased nearly three times in first generation Japanese women who had migrated to Hawaii. Additionally, they showed that in the second generation, incidence rates increased further to between four and five times. Overall, the evidence from migration studies
3 indicates that over time, changes in diet and/or environment can affect breast cancer incidence rates.
Although changes in both diet and environment occur following migration from countries with low to countries with high breast cancer incidence rates, the main factor responsible has not been determined. There is no published data, however, indicating that environmental change may be responsible for the increases in breast cancer risk. On the other hand, there is some evidence that implicates changes in diet or in cooking practices. The diets and cooking practices of migrants are known to become progressively more ‘Westernized’ following migration [7-8] and in Japan, for example, the ‘Westernization’ of diet has been found to correlate with increases in breast cancer incidence [8-9].
The Western diet is characterized by high intakes of red meat, fat, refined grains and dairy products [8]. Epidemiological evidence indicates that breast cancer is positively associated with consumption of diets high in meat and animal fat. In Europe and North America, for instance, where meat products contribute 14-15% of the dietary energy supply, while cereal and grain products only contribute 23%, the rate of breast cancer is amongst the highest in the world, while in Africa, where the cereals and grain products contribute up to 65% and meat products only contribute 2-5% of the dietary energy supply, the rate of breast cancer is relatively low [7].
Furthermore, it has recently been shown that cancer rates in cities within economically developing countries are now approximating the cancer rates of western cities. In Singapore, for example, the incidence of breast cancer approximately doubled between the 1970s and 1990s
[11]. The shift in breast cancer pattern here is thought to be a result of rapid economic development in this area, where energy dense foods such as meat and dairy products are becoming more affordable, and are replacing traditional phytochemical-rich fruits, vegetables
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and legumes. This idea is supported by data from India, where cancers associated with Western
diets are also becoming more common in the more urbanized areas of the country [12].
Numerous dietary components have been hypothesized to reduce the risk of breast cancer
[13-23]. Epidemiological evidence indicates that high levels of cruciferous vegetable intake are
associated with reduced risk of acquiring several types of cancers, including breast cancer. For
example, in a cohort study of 628 men, Cohen et al. showed that consumption of 3 or more
servings of cruciferous vegetables per week was associated with a 41% decreased risk of prostate
cancer, compared with those eating less than one serving per week [24]. Data from the Health
Professionals Follow-up Study indicates that high cruciferous vegetable consumption may
reduce bladder cancer risk, while other vegetables and fruits may not confer appreciable benefits
against this cancer [25]. Furthermore, in an analysis of 87 case-control studies, Verhoven et al showed that 67% of the studies showed an inverse relationship between consumption of cruciferous vegetables and risk of cancer at various sites (including lung, breast, and colon) [26].
Introduction to Thesis
This thesis will focus on the protective effects of cruciferous vegetable consumption.
Specifically, it will describe our investigation of the effect of the bioactive crucifer component,
indole-3-carbinol (I3C), and its derivative product, 3,3’-diindolylmethane (DIM), on the
expression of fatty acid synthase (FAS), an enzyme involved in cancer cell proliferation, in
cultured breast cancer cells.
1.1 - Cruciferous Vegetables
Cruciferous vegetables come from plants in the family known to botanists as Cruciferae
or Brassicaceae. Plants in this family have flowers with four equal-sized petals in the shape of a
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‘crucifer’ or cross. “Brassica” is the Latin term for cabbage. Many commonly consumed cruciferous vegetables come from the Brassica genus, including broccoli, Brussel sprouts, cabbage, cauliflower, bok choy, turnips, collard greens and kale. Although not in the Brassica genus, watercress, radish and arugala are also cruciferous vegetables [27].
Like other vegetables, cruciferous vegetables contain a number of components with cancer chemopreventative properties, including folate, fiber, carotenoids and minerals [27].
However, cruciferous vegetables are unique in that they are rich sources of glucosinolates. As will be discussed in the following sections, glucosinolates may play a significant role in the association between cruciferous vegetable consumption reduced cancer rates.
1.1.1 - Glucosinolates
Glucosinolates are a class of organic compounds that give cruciferous vegetables and some condiments, such as wasabi and mustard, their pungent aromas and spicy (some say bitter) taste. The main function of glucosinolates in plants is as natural pesticides and as a defense against herbivores [28].
Figure 1.1: General chemical structure of a glucosinolate molecule
Over 120 different glucosinolates have been identified [27]. Figure 1.1 shows the general chemical structure of glucosinolate molecules. The central carbon of all glucosinolates is bound
6 to a thioglucose group to a sulfate group via the nitrogen atom. The central carbon of each glucosinolate is also bound to a side group (designated R in Figure 1.1), and this is what makes each glucosinolate unique. The R-group is derived from protein amino acids and the diversity of glucosinolates is obtained by secondary modifications of the side chain and/or glucose moiety.
Glucosinolates are classified as aliphatic (e.g. alkyl, alkenyl, hydroxyalkenyl or w- methylthioalkyl), aromatic (e.g. benzyl, substituted benzyl) or heterocyclic (e.g. indolyl) [29], with the R-group of the aliphatic glucosinolates being derived from methionine, alanine, leucine or valine; and those of aromatic and heterocyclic glucosinolates being derived from tryptophan, phenylalanine or tyrosine.
Worldwide, cruciferous vegetable intake varies. It has been estimated that on average,
North Americans consume 14.7mg of glucosinolates from cruciferous vegetables daily [30]. On the other hand, in Japan, a country associated with lower incidence of several cancers (including breast cancer), it has been estimated that glucosinolate consumption from cruciferous vegetables averages 112mg per day [31]. However, it should be noted that in Japan, radishes are the primary source of glucosinolates, as they make up more than 1% of all food sold.
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Table 1.1: Food sources of selected glucosinolates and their hydrolysis products that are currently under investigation for their cancer chemopreventative properties.
Each cruciferous vegetable contains a mixture of glucosinolates. Table 1.1 lists a number of cruciferous vegetables and the glucosinolates they contain. A number of comparative studies of glucosinolate distribution and variability between specific cruciferous vegetables have been performed. These studies have compared the glucosinolate levels in the edible portions of some of the most widely consumed cruciferous vegetables and suggest there are considerable differences in the glucosinolate levels between each type of crucifer. For example, Carlson et al
[32] reported 13 different glucosinolates in broccoli, Brussel sprouts, cauliflower and kale. The authors also showed that certain cultivars were highly correlated in their glucosinolate pattern and could be grouped together. Broccoli, for instance, formed one group with higher levels of glucoraphinin; Brussel sprouts and cauliflower with higher levels of glucobrassicin formed a second group; collard greens with higher levels of progoitrin formed a third group, and mustard greens with higher levels of sinigrin formed a fourth group. Radishes are a rich source of glucoraphasatin. Similar studies have since been performed comparing a wider array of crucifers and have demonstrated that the glucosinolate content of each cruciferous vegetables varies -
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where each type of cruciferous vegetable contains higher levels of certain glucosinolates and
lower levels of other glucosinolates [33-34].
Additionally, it has been determined that glucosinolate levels in crucifers are also affected by the growing location. Shelp et al. [35] evaluated glucosinolate distribution in two broccoli cultivars grown at three different locations. They reported that differences in glucosinolate content among growing sites were greater than differences between cultivars.
Factors that may have contributed to these differences included soil type, sulphate and nitrate fertilizer application, plant spacing and date of harvest. Higher levels of glucosinolates were found in plants grown on clay soil than on sandy soil and in plants treated with sulphate than in
plants treated with nitrate. Hence, environment and factors associated with culture conditions
significantly influence cruciferous vegetable glucosinolate distribution.
1.1.2 - Activation of Glucosinolates by Myrosinase
Although glucosinolates are associated with inhibition of carcinogenesis, it is actually
their hydrolysis products, not the glucosinolates themselves that are biologically active.
Hydrolysis of glucosinolates is catalyzed by the enzyme myrosinase, also known as β-
thioglucoside glucohydrolase [28]. Glucosinolates co-exist with myrosinase in cruciferous
vegetables; however, the two are kept apart from each other as myrosinase is stored in
specialized cells known as myrosin cells. Upon wounding of the vegetable, for example, after
chopping, crushing, chewing or freeze-thawing, myrosinase may be released from the myrosin
cells. Myrosinase then acts by cleaving glucsinolates at their thioglycoside linkage to produce
glucose and an unstable aglycone thiohydroximate-O-sulfonate, which, in turn, spontaneously
rearranges to yield an isothiocyanate, nitrile or thiocynate product (Figure 1.2) [29].
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Figure 1.2: Bioactivation of glucosinolates. Hydrolysis of glucosinolates by myrosinase to form nitriles, thiocyanates and isothiocyanates [image taken from ref 8].
The extent of hydrolysis of glucosinolates by plant myrosinase and the structure and
concentration of metabolites formed is influenced by various features of the hydrolysis
environment (such as the presence of ascorbic acid or Fe2+, and extrinsic factors such as pH and
temperature) [36, 37].
1.1.3 - Factors Influencing Myrosinase Activity
Several factors influence the glucosinolate-myrosinase hydrolysis reaction. Indeed, the activity of myrosinase can vary extensively between and within brassica species and in different parts of the plant [37]. However, cruciferous vegetables undergo a variety of post-harvest
processes, including storage, preparation and cooking, before they are consumed. During these
stages myrosin cells may deteriorate and the concentration of glucosinolates becomes altered, as
10 the bioactive glucosinolate products themselves deteriorate after a few days [38]. This, in turn, leads to considerable uncertainty in assessing rates of exposure to glucosinolates and their metabolites at target tissues.
Upon cooking cruciferous vegetables, the glucosinolate-myrosinase system can further become altered as a result of partial or total inactivation of myrosinase, thermal or plant myrosinase mediated breakdown of glucosinolates, loss of enzymatic cofactors, leaching of glucosinolates and their metabolites into the cooking medium or thermal degradation of the metabolites. These changes are mostly influenced by the duration and method of cooking, the type of vegetable matrix and the extent of its cellular disruption, and the chemical structure of the glucosinolate precursors [38]. Furthermore, the thermostability of myrosinase varies depending on the crucifer source. For example, myrosinase extracted from broccoli loses approximately 90% of its activity after heating at 60oC for 3 minutes at pH 6.5, whereas 30 minutes of heating homogenized red or white cabbage at pH 7 and 70oC is required to reduce its myrosinase activity by 90% [37, 39-40].
Following ingestion, a second phase of hydrolysis of glucosinolates may occur in the gastrointestinal tract under the action of the colonic microflora. Intestinal microflora that come in contact with intact glucosinolates activate them by digesting the glucosinolates themselves, cleaving the glucosinolate at its thioglycoside linkage, to produce the bioactive compound. The digestive and post-absorptive fate of glucosinolates in vivo may be influenced by factors such as the activity of plant myrosinase ingested, the extent of chewing, the nature of the meal containing the crucifers, the composition of the gut microflora and genotypic variation in post- absorptive metabolism [41-42].
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1.1.4 - Bioactive Glucosinolate Products
As mentioned above, myrosinase-mediated glucosinolate hydrolysis reactions yield
products shown to have cancer chemopreventative properties. For example, gluconasturiin, the
major glucosinolate of watercress, is the precursor of phenethyl isothiocynate (PEITC) [56]. In
vitro, PEITC induces apoptosis of MCF-7 human breast cancer cells, and has been shown to inhibit tumorigenesis in rodents [43-46]. Glucoraphinin, a major glucosinolate in broccoli, is the precursor of sulforaphane (SFN), that like PEITC, also exerts cancer preventative properties such as the induction of apoptosis and the reduction of cellular proliferation of various cancer cell lines [43, 47-49]. Table 1.1 lists other isothiocyanates and indoles that are currently under investigation for their cancer chemopreventative properties, along with their glucosinolate precursors.
1.2 – Indole-3-Carbinol (I3C) and 3,3’–Diindolylmethane (DIM):
One of the most extensively studied glucosinolate hydrolysis products known to have
anticancer effects is indole-3-carbinol (I3C), also called 3-(hydroxymethyl)-indole (Figure). I3C
can be derived from several cruciferous vegetables (including broccoli, Brussel sprouts and
cabbage) and is produced by the hydrolysis of glucobrassicin [27].
In a low pH environment, such as that in the stomach, I3C is converted to a number of
oligomeric products (Figure 1.3a). It has been suggested that the observed biological activity of
I3C may be attributable mainly to the acid condensation products, in particular, 3,3’–diindolyl- methane (DIM) (Figure 1.3b). DIM is the major in vivo I3C derivative making up 5.9-11% of the total amount of I3C condensation products in the stomach [50].
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Figure 1.3: Molecular structures of (a) I3C and (b) DIM
Both I3C and DIM are known to have chemopreventative properties. The following section will discuss I3C intake levels, I3C and DIM tissue distribution levels, physiologically relevant in vitro doses of I3C and DIM, and will review much of the existing literature on the effect of I3C and/or DIM on cancer.
1.2.1 – Tissue Distribution, Intake Levels and Physiologic Concentrations
The tissue distribution of I3C has been determined in mice using radio-labelled I3C. Both
I3C and DIM have been detected in liver, kidney, lungs, heart, plasma and brain samples of mice treated with 250mg/kg of I3C as early as 15 minutes after administration [69]. These results suggest that I3C is rapidly absorbed and distributed to a number of well-perfused tissues, where it is converted to DIM to perform its anticancer actions.
Plasma and tissue levels of I3C and DIM have been extrapolated from animal studies, since levels for humans are not available. Mice fed 250mg/kg of I3C produced maximum concentrations of 29 and 170 μM I3C in their plasma and liver, respectively (15 min). I3C produced maximum concentrations of 4 and16 μM DIM in their plasma and liver, respectively
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(after 2 h) [52]. By allometric scaling, Howells et al. have determined the I3C dose given to mice would equate to a 20mg/kg dose in humans (or 1.2g of I3C/d). To achieve intake, I3C must be taken as a supplement, since dietary intake of glucobrassicin, the precursor of I3C in cruciferous vegetables is much lower. In the United States and the United Kingdom, estimated per capita intakes of glucobrassicin are 8.1 and 19.4mg/d, respectively [53,54], whereas in some populations in Asia, the level reaches 46mg/d [55]. As will be further explained below, I3C, taken as a supplement, has been shown to have chemopreventative effects at doses ranging between 200-800mg/d.
In vitro studies, many of which are mentioned below, that have investigated the mechanisms involved in the anticancer effect of I3C have treated cells with doses of I3C ranging from 10 nM to 250 μM. Howells et al. have reviewed a number of in vivo and in vitro studies to determine physiologically relevant in vitro doses of I3C and DIM. They suggest that serum concentrations of up to 150 µM for I3C and 50 µM for DIM are physiologically relevant to humans [52]. These concentrations have been considered in the design of our in vitro studies.
1.2.2 – Cancer Protective Effects of I3C and DIM in Rodents
I3C in Rodents
It has been demonstrated that I3C is active against a number of carcinogen-induced and spontaneous tumors in multiple tissues in rodents.
Breast Cancer - Several studies have evaluated the efficacy of I3C in the prevention of chemically-induced mammary tumors. Using the 7,12-dimethylbenz[α]anthracene (DMBA)- model, Grubbs et al [56] have shown that mammary tumor multiplicity may be reduced by 91-
96% in Sprague-Dawley rats after administration of 50mg I3C/kg of diet per day five times a week during the initiation phase. Similarly, 50mg I3C/kg of diet given both prior to and after
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treatment with MNU (a direct acting carcinogen) caused a 65% decrease in mammary tumor
multiplicity in Sprague Dawley rats [56]. Bradlow et al [57] have shown that C3H/OuJ mice
given diets containing 500-2000 ppm I3C for 8 months have significantly lower spontaneous
mammary tumor incidence and multiplicity compared to those given the a diet without I3C.
Furthermore, the mice given the high I3C dose also had a prolonged tumor latency.
Liver Cancer – I3C supplementation has effectively reduced tumor formation in liver.
Manson et al [58] have shown that I3C (making up 0.5% of the diet) fed to male Fischer rats 2
weeks prior to administration of aflatoxin B1 reduced the development of preneoplastic hepatic
lesions by 53%.
Lung Cancer - Morse et al [59] showed a 40% inhibition of NNK- induced pulmonary
adenoma multiplicity (NNK is 4-(methylnitrosamino)-1-(3-pyridyl)-1-butanone, an important lung carcinogen present in tobacco smoke) in A/J mice pre-treated with I3C. In a similar study,
Kassie et al [60] tested the chemopreventative efficacy of I3C against lung tumorigenesis induced by a mixture of NNK and benzo[a]pyrene (BaP) in A/J mice. They showed that of 112
μg I3C/g of diet for 23 weeks resulted in a reduction of lung tumor multiplicity by 86%.
Furthermore, compared to the lung tissues of untreated mice, I3C inhibited expression of SP-C,
L-plastin, annexin A1, and haptoglobin – several proteins associated with lung cancer. In addition, I3C was shown to suppress breast cancer cell metastases, as well as inhibit the formation of lung surface metastatic nodules when poorly invasive MCF-7 or highly invasive
MCF-468 cells were injected intravenously into mice.
Tongue Cancer - Tanaka et al [61] have shown that a diet containing I3C at a dose of
1000 ppm inhibits 4-nitroquinoline 1-oxide (4NQO-) induced neoplasm formation in ACI/N rat tongues, when given during both the initiation and post-initiation phases of carcinogenesis.
15
Endometrial Cancer - Kojima et al [62] showed that a diet containing 1000 ppm I3C resulted in a 44% reduction in the occurrence of spontaneous endometrial adenocarcinomas in
Donryu rats.
Cervical Cancer – Transgenic mice expressing the human papillomavirus type 16 under a keratin 14 promoter (K14-HPV16 mice), developed cervical cancer when they were given 17β- estradiol chronically. Jin et al [63] showed that mice fed I3C at a dose of 2000ppm in the diet had a 68% lower in cervical-vaginal cancer incidence after 6 months compared to the unsupplemented group. Furthermore, they showed that I3C prevented morbidity associated with retention of fluid in the bladder that frequently occurred with the higher estradiol dose.
Additionally, I3C appeared to reduce skin cancer in the transgenic mice.
DIM in Rodents
Several studies have been published on the effect of DIM on carcinogen-induced tumors in rodents. As with I3C, the results from the existing data appear promising as they provide evidence of a strong protective effect for DIM against the formation of certain cancers.
Breast Cancer – Chen et al [64] showed that administration of 5 mg/kg DIM every other day for a total of 20 days significantly inhibited DMBA-induced mammary tumorigenesis in female Sprague–Dawley rats. Using a complementary in vivo Matrigel plug angiogenesis assay,
Chang et al [65] have demonstrated that, compared with vehicle control, neovascularisation of mammary tumors in female C57BL/6 mice may be inhibited by up to 76% following the administration of 5mg/kg DIM. Furthermore, they have shown that this dose of DIM also inhibits the growth of human MCF-7 cell tumor xenografts by up to 64% in female athymic (nu/nu) mice compared to vehicle control [66]. Finally, McDougal et al [67] have shown that DIM significantly inhibits mammary tumor growth in female B6C3F1 mice implanted with a T47D
16
(estrogen sensitive human breast cancer cell line) xenograft, at a low DIM dose of 1mg/kg of
body weight.
Colon cancer – In an azoxymethane (AOM)-initiated colon carcinogenesis model, Kim et
al [68] have showed that DIM administration dramatically decreased the number of colon tumors
in BALB/c mice treated with 20mg DIM/kg. Furthermore, the antiinflammatory effects of DIM
in dextran sodium sulfate (DSS)-induced colitis was also inestigated in this study, and it was
shown that DIM significantly attenuated the loss of body weight and shortening of the colon -
two severe symptoms in this colitis model. Furthermore, they showed an associated reduction in
the disruption of the colonic architecture, a significant reduction in colonic myeloperoxidase
activity and production of prostaglandin E(2), nitric oxide, and proinflammatory cytokines – all
of which contribute to colitis.
Lung Cancer - In a follow-up to the study described for I3C in the previous section,
Kassie et al [69] tested the efficacy of DIM against lung tumorigenesis induced by a mixture of
NNK and benzo[a]pyrene (BaP) in A/J mice. They showed that DIM at 30 μg/g of diet for 23
weeks resulted in a reduction of NNK plus BaP-induced lung tumor multiplicity by 66%. They showed differences in the relative abundance of proteins associated with lung tumors in the pulmonary tissues of carcinogen-treated versus untreated mice. Specifically they found that fatty acid synthase, transketolase, pulmonary surfactant-associated protein C (SP-C), L-plastin,
annexin A1, and haptoglobin increased, whereas transferrin, alpha-1-antitrypsin, and apolipoprotein A-1 decreased.
Prostate Cancer – Nachshon-Kedmi et al [70] have demonstrated that DIM given to male
C57BL/6 mice 3 times a week for 3 weeks at doses of 2.5-10mg/kg body weight inhibits tumor growth of TRAMP-C2 (a mouse prostate cancer cell line) xenografts by up to 46%, compared to
17
vehicle control. Histological examination of the tumors from treated groups revealed increased
apoptotic activity and decreased cell proliferation compared with the control tumors.
1.2.3 – Cancer Protective Effects of I3C and DIM in Humans
In humans, the bioavailabilities of I3C and DIM have not been determined. As well, no
studies have been published on the in vivo effect of DIM in humans [52]. However, phase I and
phase II clinical trials have shown that orally administered I3C and/or its acid-condensation products have dose-dependent anticancer effects [71-73]. For example, female subjects with
cervical intraepithelial neoplasia (CIN) or vulval intraepithelial neoplasia (VIN) treated with
either 200 or 400 mg/d of I3C showed complete regression of CIN after 12 weeks of treatment
compared to placebo groups [74-76].
In vivo, estrogen is metabolized to several hydroxylated forms. The 2-OH derivative is
the protective, less potent estrogen; while, 16-OH estrogen, the potent form of estrogen,
increases estrogenic effects (e.g. breast cell mitosis) and accumulation of it is associated with
high risk of breast cancer. I3C treatments of 200-800 mg/d have been shown to significantly
elevate the 2-hydroxyestrone to 16α-hydroxyestrone ratio in these women compared to placebo
group, the degree of elevation depending on the administered dose [72,74].
1.2.4 – Anticancer Effects of I3C and DIM in vitro: Possible Mechanisms of Action
I3C and DIM have been studied in a number of cell lines. Both I3C and DIM have been
shown to modify nuclear transcription factors (e.g. ER, AhR, NFκB and Sp1) involved in cancer-
related cell processes including xenobiotic metabolism, cell cycle progression, proliferation
apoptosis and metastasis. This section will review the mechanisms through which I3C and DIM
have been shown to exert their anticancer effects.
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Estrogen Receptor (ER)
Estrogens exert their effects by binding to estrogen receptors (ERs). Within the nucleus, the estrogen-ER complex can bind to DNA sequences in genes known as estrogen response
elements (EREs), and enhance the transcription of estrogen responsive genes.
When added to breast cancer cells in culture, I3C has been found to inhibit cell
proliferation. The decreased proliferation occurs because I3C modifies the ER phospholylation
and DNA binding domains, which in turn, inhibits the transcription of estrogen-responsive genes
[77]. Meng et al have shown a dose-dependent repression in estrogen activated ER signaling and transcriptional activity when I3C is added to MCF-7 cells at 10-125µM [78]. Similarly, DIM has been shown to interfere with ER-DNA binding, signaling and ER expression [79,80].
Estrogen dependent genes essential for tumor cell viability, such as epidermal growth factor receptor (EGFR) in breast cancer, have been shown to decrease with I3C and DIM treatment (75 µM and 25 µM, respectively) [81, 82]. Similarly, I3C (50 µM) has been shown to inhibit phosphoinositide-3-kinase (PI3K), resulting in the inhibition of protein kinase B (Akt) phosphorylation and decreased survival of cancer cells dependent on this pathway [83]. As well, breast cancer susceptibility proteins (BRCA1/2) have been shown to be upregulated after
I3C/DIM treatment, and a mechanism involving ER modification by I3C/DIM has been proposed [77]. Hence, the anticancer effect of I3C/DIM can partly be explained by its ability modify the ER, which leads to changes in the expression of genes that inhibit cellular proliferation and promote apoptosis.
The Aryl Hydrocarbon Receptor (AhR)
The AhR is a nuclear transcription factor that can be activated in the cytoplasm by binding to several types of aromatic compounds (e.g. dioxins, flavonoids) including I3C and
19
DIM [77]. Binding allows the AhR to enter the nucleus where it forms a complex with the AhR
nuclear translocator (Arnt) protein. This Ahr/Arnt complex binds to specific DNA sequences in
genes known as xenobiotic response elements (XRE) and enhances their transcription. Genes for
a number of CYP (e.g. CYP1A1, CYP1B1) enzymes and several phase II enzymes (e.g.
glutatione-S-transferase) are known to contain XREs. By increasing the activity of
biotransformation enzymes, I3C and DIM are thought to exert part of their anticancer effect by
enhacing the metabolism or elimination of potential carcinogens or toxins [52].
As mentioned above increased levels of circulating 16-OH estrogen is known to enhance
breast cancer cell proliferation and tumorigenesis [77]. Steroid hydroxylases related to CYP1A1
catalyze the formation of 2-OH estrogen, and can increase the ratio of circulating 2-OH:16-OH
estrogen [52]. Ociepa-Zawal et al. have shown that MCF-7 cells increase transcription and
activity of CYP1A1 following 48 hour treatment with 100µM I3C [84], while Chen et al [64]
have similarly shown that 24 hour treatment with DIM at 50 µM induces CYP1A1 gene
expression in these cells. As well, rats given I3C or DIM have been shown to increase the
capacity of hepatic microsomes to convert estrogen to 2-OH estrogen and increased expression
of CYP1A1 [85]. Hence, part of the protective effect of I3C and DIM includes its influence on
the AhR to induce hormone and xenobiotic metabolism.
Nuclear Factor κB (NFκB)
The anticancer effect of I3C and DIM has also been suggested to be partly due to an increase in cell apoptosis (programmed cell death). NFκB is a transcription factor that has an important role in regulating the genes involved with the apoptotic process. NFκB binds to the promoter region of the Bcl-2 gene (antiapoptotic protein) and allows its expression. When NFκB expression is inhibited, Bax (a proapoptotic protein) is released from the Bax/Bcl-2 dimer and
20
can induce apoptosis [77]. Studies with several breast cancer lines indicate that the relative
amounts of Bax and Bcl-2 proteins are highly predictive of sensitivity to apoptosis in mammary
tumor cells.
Translocation of Bax protein from the cytosol to the mitochondria results in
mitochondrial depolarization and the release of apoptosis associated factors in the mitochondria
(e.g. apoptosis-protease-activated factor 1, apoptosis-inducing factor 1 and cytochrome c) [77].
Rahman et al. [86] showed that apoptosis was induced in MCF-7 cells treated with 60 µM I3C for 48 h, with an associated decreased level of Bcl-2. Similarly DIM has been shown to increase the Bax/Bcl-2 ratio in MCF-7 cells [87]. Hence, I3C/DIM modulates apoptosis by inhibiting the
activation of NFκB, which allows for the release of apoptosis associated factors resulting from
increased levels of free mitochondrial Bax.
Specificity Protein 1 (Sp1)
I3C and DIM have been shown in vitro to modulate nuclear transcription factors that are involved in regulating downstream cellular events such as cell cycle progression. The nuclear transcription factor specificity protein 1 (Sp1) is a sequence-specific DNA-binding protein that activates a broad and diverse spectrum of mammalian and viral genes. It acts by recognizing GC- rich promoter elements and interacting with DNA through three zinc fingers located at the C- terminal domain, leading to expression of those genes [88]. In cancer, Sp1 protein plays a critical role in the growth and metastasis of many tumor types by regulating expression of cell cycle genes [77].
I3C and DIM have been shown to regulate expression of cyclin-dependent kinase 6
(CDK6), an enzyme involved in cell cycle control, in MCF-7, MDA-MB231 and LNCaP cells.
I3C/DIM disrupts the interactions of Sp1 with its DNA-binding site within the CDK6 promoter,
21
leading to suppression of CDK6 expression and cell cycle arrest at the G1 phase [89-92].
Similarly, MCF-7 and MDA-MB231 cells treated 50uM DIM for 48 hours have decreased expression of CDK6 and G1 cell cycle arrest [122, 124-125]. Futhermore, it has also been shown
that the G1 cell cycle arrest is due to elevated p21 levels (a CDK inhibitor). DIM is thought to
induce the binding of Sp1 to the Sp1-responsive elements of p21 in its promoter region, thereby
increasing p21 expression in MCF-7 cells [89]. Hence, by modifying Sp1 binding, I3C/DIM acts
on cancer cells to arrest cell cycle progression and decrease the proliferation rate of cancer cells.
The relationship between I3C/DIM, Sp1 and proliferation will be further explored in
relation to my thesis experiments in the next section.
Metastasis
I3C has also been shown to affect breast cancer cell motility. Brew et al [93]
demonstrated that 100uM I3C significantly decreases in vitro migration of MDA-MB231 cells -
an indole-sensitive, highly invasive breast cancer cell line. I3C treatment activates Rho kinase
activity in these cells, resulting in the formation of localized stress fibers and peripheral focal
adhesions, which decrease overall cell motility.
Furthermore, elastase (an intracellular protease) activity has been shown to be inhibited
in MDA-MB231 cells treated with 100uM I3C [94]. High elastase activity is a marker for breast
cancer survival and metastasis progression. Inhibition of elastase causes the accumulation of 50- kDA cyclin E and loss of 35kDA cyclin E (the larger form is typically expressed in normal mammary tissue, while the smaller form is associated with poor clinical outcomes). Disruption of the proteolytic processing of the 50-kDA cyclin E into the smaller form by I3C inhibits cell cycle progression and cell motility. This inhibition effect of I3C on elastase, however, is specific to I3C since 50 μM DIM did not produce similar results [94].
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1.3 - Fatty Acid Synthesis
Fatty acid synthesis is a biochemical process common to all animals that converts excess
dietary glucose to the non-essential fatty acid palmitate. The process begins with glycolysis
(Figure 1.4). Glucose is converted to glucose-6-phosphate by hexokinase, which then enters the glycolytic pathway to generate pyruvate, the major glycolytic end-product, and ATP. Cancer cells produce excess pyruvate as they have an elevated rate of glucose catabolism compared to non-cancer cells [95]. Most pyruvate is converted to lactate in the cytoplasm by lactate-
dehydrogenase and is secreted from the cell; however, some pyruvate is taken up by the
mitochondria and enters the citric acid cycle, producing acetyl coenzyme A (CoA) [96].
In the mitochondria, acetyl CoA is converted to citrate, that can be transported to the
cytosol by tricarboxylate translocase. Citrate, in the cytoplasm, is then converted back to acetyl-
CoA by ATP citrate lyase (ACL), where a portion of it is carboxylated to malonyl-CoA by
acetyl-CoA carboxylase (ACC). Fatty acid synthase (FAS) then performs the condensation of
acetyl-CoA and malonyl-CoA (and NADPH as a reducing agent) to produce palmitate, a 16-
carbon saturated fatty acid (further described below), and other saturated long-chain fatty acids.
Saturated long-chain fatty acids may further be modified by elongases (in the
mitochondria and endoplasmi reticulum) or desaturases to form more complex fatty acids, that
may be used for the synthesis of various cellular lipids such as phospholipids, triglycerides and
cholesterol esters [96].
23
Figure 1.4: Glycolysis and fatty acid synthesis .[image taken from ref 95]
1.3.1 - Fatty Acid Synthase (FAS) and de novo Generation of Palmitate
Of the various enzymes mentioned in the previous section, FAS is the major biosynthetic
enzyme involved in de novo palmitate synthesis. FAS may also produce smaller amounts of myristate, laureate, and even shorter-chain fatty acids. Two kinds of FAS proteins are classically
recognized: cytosolic FAS (FAS I) and mitochondrial FAS (FAS II). Cytosolic FAS is primarily
responsible for de novo fatty acid synthesis, whereas mitochondrial FAS provides octanoyl
precursors required for the essential lipoylation pathway [97,98].
Mammalian FAS consists of two identical multifunctional 250 kDa polypeptides. The monomers are arranged in a head-to-tail configuration and are held together by two thio-disulfide
24
bonds. Each monomer includes seven catalytic domains, and each of the domains has a distinct
activity required for fatty acid biosynthesis [95]. The enzymes in the FAS complex include:
malonyl/acetyl-CoA-ACP transferase (MAT), β-ketoacyl synthase (KS), β-ketoacyl-ACP
reductase (KR), β –hydroxyacyl-ACP dehydrase (DH), enoyl-ACP reductase (ER) and palmitoyl
thioesterase (TE). The clustering of the domains in FAS offers great efficiency and coordination
during palmitate synthesis [96].
The reactions catalyzed by each domain in mammalian FAS are illustrated in Figure 5.
Synthesis of palmitate begins with the “loading” of FAS with malonyl-CoA. The malonyl group
originally linked as a thioester in malonyl-CoA, is first transferred first to the anchoring protein
acyl-carrier protein (ACP) (1) and then to the Cys residue KS enzyme to form malonyl-ACP, the
growing fatty acid (2a). Similarly, an acetyl group is transferred from acetyl-CoA to ACP to
form acetyl-ACP (2b).
In the next step (3), known as the condensation reaction, malonyl-ACP is decarboxylated, driving a resulting carbanion to attack the acetyl-thioester. This reaction, in turn, results in the formation of a four-carbon β-keto-ACP.
Two reductions and a dehydration (4-6) then convert the β-keto group to an alkyl group, where the coenzyme in both reductive steps is NADPH. Here, NADPH is provided in a reaction catalyzed by malic enzyme or can be acquired through the pentose phosphate pathway.
At this point, the acyl group, originally an acetyl group, has been elongated by a C2 unit.
The butyryl group is then transferred from ACP to the Cys-SH in the KS domain (a repeat of
2b). In each reaction cycle, the ACP is “reloaded” two carbon atoms. Seven such cycles are required to form palmitoyl-ACP. The thioester bond is then hydrolyzed by palmitoyl thioesterase
(7), yielding palmitate, and regenerating the enzyme for a new round of synthesis [98].
25
1
2a 2b
3
4
5
6
7
thioesterase
Palmitate
Figure 1.5: Palmitate synthesis in FAS enzyme complex [image taken from ref 98]
26
1.3.2 - FAS in Normal Tissues
FAS expression varies in a tissue specific manner. Most normal tissues, such as the skin
or skeletal muscle, express FAS at low levels and synthesize low levels of palmitate [99]. Cells
from these tissues acquire fatty acids from circulating levels made available by the diet rather
than via de novo synthesis.
Liver and adipose tissues, on the other hand, are highly lipogenic tissues and express FAS
at relatively higher levels. Fatty acid synthesis in adipose tissue, for example, occurs 10-1000
times more rapidly than it does in skeletal muscle cells [101]. In adipose, FAS functions to
maintain energy balance for the organism, converting excess calories from the diet into storage
lipid. In the liver, FAS functions to synthesise fat from protein and carbohydrate when dietary
sources of fat are lacking.
In mammals, expression of FAS in certain tissues also depends on stage in development.
For example, in the maturing fetal lung, FAS is elevated to provide the fetus with palmitic acid
for the synthesis of lecithin. After birth, FAS levels in the lungs of newborns lower and steadily
plateau to adult lung levels. Similarly, during lactation, FAS is elevated in the mammary gland to
supply medium chain fatty acids, such as myristate, for breast milk [101]. As the frequency
breast-feeding decreases, FAS levels in the mammary gland also decrease.
Few diseases directly involve the fatty acid synthesis pathway, although variations of
FAS activity may have an influence on diseases such as obesity and diabetes. Nonetheless, fatty acid synthesis has been shown to be crucial for development. In mice, FAS homozygous knockouts are non-viable, with most of the embryos dying before implantation [101]. As well, most heterozygous FAS knockout mice die at various stages of embryonic development [102].
Surviving heterozygous mice possess 50% and 35% lower FAS mRNA and activity compared to wild types, suggesting that the lack of FAS gene has significant teratogenic consequences.
27
Additionally, conditional knockout FASKOL (FAS knockout in liver) mice develop fatty livers
and liver disease when consuming fat free diets [103]. In these mice, fatty acids are mobilized
from the adipose tissue to the liver. However, due to the liver’s inability to synthesize new fatty
acids, the incoming fatty acids are not oxidized and build up. This suggests that FAS, is
necessary to maintain normal health and that a basal level of de novo fatty acid synthesis is
required.
1.3.3 - Inhibitors of FAS
A number of molecules that target FAS and inhibit its activity exist in nature or have
been developed.
Cerulenin
Cerulenin ([2S,3R] 2,3-epoxy-4-oxo-7E,10E-dodecadienamide) is an antifungal antibiotic found naturally in the industrial strain of the fungus cephalosporium ceruleans [104].
Cerulenin covalently binds to the FAS β-ketoacyl synthase moiety, thus preventing the condensation reaction between the elongating fatty acid chain and successive acetyl or malonyl residues [105]. In vitro, cerulenin causes dose-dependent decreases in cell proliferation of breast, ovarian, prostate and colon cancer cells [106-108]. Pro-apoptotic effects have been shown in colon cancer cells as well [109]. The clinical relevance of cerulenin, however, is limited because of the chemical instability caused by its very reactive epoxy group. Furthermore, its been demonstrated that a dose of 30 milligrams per kilogram of cerulenin inhibits feeding and induces dramatic weight loss of mice by a mechanism similar to, but independent of, leptin signaling
[110].
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C75
C75 (4-methylene-2-octyl-5-oxotetrahydrofuran-3-carboxylic acid) is a cerulenin-derived
semi-synthetic FAS inhibitor. Like cerulenin, C75 covalently binds to the FAS β-ketoacyl
synthase moiety and prevents the condensation reaction. Unlike cerulenin, C75 lacking the
reactive epoxy group making it a more stable and effective treatment [111]. C75 also increases
activity of carnitine palmitoyltransferase-1 (CPT-1), an enzyme involved in fatty acid oxidation; hence, making it a more potent weight-loss-promoting drug than cerulenin. Both lean and obese
mice treated with C75 undergo rapid and profound weight loss and loss of adipose mass [112].
Furthermore, cells and mice treated with doses of C75 as low as 10uM have shown cytotoxic
effects [113]; hence, precluding it from being developed as a safe drug.
Orlistat
The β-lactone Orlistat (1-(3-hexyl-4-oxo-oxetan-2-yl)tridecan-2-yl 2-formylamino-4- methyl-pentanoate) is a US FDA-approved anti-obesity drug [114]. Orlistat elicits its effect by blocking the palmitoyl thioesterase domain in the FAS complex, which is responsible for releasing palmitate from FAS [115]. Orlistat has been shown to arrest proliferation and induce apoptosis of LNCaP, DU-145, and PC-3 prostate cancer cell lines [116]. Furthermore, it has been shown to inhibit growth of PC-3 tumors in male athymic nude mice [115]. Clinically, however,
Orlistat has poor solubility and low oral bioavailability [117]; hence, it may not necessarily be able to act on tumors other than those confined to the gastrointestinal tract.
Triclosan
Triclosan (2,4,4’-trichloro-2’-hydroxydiphenyl ether) is a widely-used antibiotic in soaps, mouthwashes and other oral health care products, and blocks FAS activity by inhibiting the
29 enoyl-ACP reductase domain [118]. Triclosan has been shown to inhibit MCF-7 and SKBr-3 proliferation by as much as 50% when given at a concentration of 50 uM [119]. A diet containing 1000 ppm triclosan has been shown to suppress MNU-induced-mammary carcinogenesis of Sprague-Dawley rats [120]. Furthermore, acute, subacute/subchronic, and chronic toxicity tests have determined that triclosan is neither an acute oral toxicant nor that it acts as a carcinogen, mutagen, or teratogen [121]. However, triclosan has been associated with side effects, the major one being that it disrupts the colonic bacteria of rats, dogs and rabbits.
Dietary compounds
Several dietary compounds have been shown to reduce FAS activity. For example, epigallocatechin-3gallate (EGCG), a component of green tea, acts similarly to cerulenin and C75 by blocking the FAS KS domain [122]. Other EGCG-related naturally occurring polyphenols
(the flavonoids luteolin, quercetin, and kaempferol) also block FAS KS activity [123]. Water- soluble organosulfur compounds of garlic have been shown to inhibit FAS activity by inhibiting the enoyl-ACP reductase domain, similarly to triclosan [124]. Furthermore, a diet given to male
Wistar containing 0.2% dietary sesamin, the most abundant lignin in sesame seeds, results in the reduction of both FAS activity and mRNA levels [125]. As well, rats consuming a diet containing 0.2% curcumin, a bioactive component in turmeric, have reductions in their hepatic
FAS activity [126]. And finally, extracts from traditional Chinese medicinal herbs such as ginko leaf and fleeceflower root have also been shown to directly inhibit FAS activity in MDA-MB435 breast cancer and PC-3 prostate cancer cell lines [127].
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1.3.4 - Regulation of FAS
Regulation of FAS may be classified as either short-term (minutes to hours) or long-term
(hours to days). Short-term regulation usually involves modification of FAS enzyme activity,
while long-term regulation refers to the regulation of FAS at its mRNA expression or enzyme
synthesis/breakdown level.
1.3.4.1 - Short-term regulation
In normal tissues, FAS activity in the short-term is regulated by circulating fatty acids and by hormones affected by the diet (i.e insulin and glucagon). During fasting, for example, as insulin and free fatty acid levels decrease in the blood, while glucagon, epinephrine and norepinephrine levels rise. The increasing concentration of these hormones causes an elevation of cAMP levels in the lipogenic tissues (i.e. the liver and adipose). cAMP is an allosteric activator of cAMP-dependent protein kinase (cAPK), which, in turn, phosphorylates and
activates several enzymes in the β-oxidation pathway including hormone-sensitive
triacylglycerol lipase (HsTL) in the liver and adipose tissue. (HsTL frees fatty acids for
metabolism by the liver and muscle). cAPK also inactivates acetyl-CoA carboxylase – the
enzyme that converts acetyl-CoA to malonyl CoA - reducing the level of substrate available for
palmitate synthesis by FAS [128]. Therefore, during fasting, glucagons, epinephrine and
norepinephrine signals cause a reduction in FAS activity by limiting the amount of available
malonyl-CoA levels.
On the other hand, during the fed state, as free fatty acid and insulin levels in the blood
rise, FAS activity in the liver and adipose increase compared to the fasting state. Insulin has the
opposite effect of glucagon, epinephrine and norepinephrine: it decreases cAMP levels, leading
to a reduction in cAPK production. A reduction in cAPK leads to the dephosphorylation and
31
inactivation of of HsTL, decreasing the amount of fatty acids available for oxidation. More
importantly, less cAPK also results in the activation of acetyl-CoA carboxylase. This leads to
increased malonyl-CoA synthesis, which in turn, increases the amount of substrates availability
for palmitate synthesis by FAS [128]. Therefore, during the fed state, insulin signals increase
FAS activity by elevating the amount of available malonyl-CoA levels.
1.3.4.2 - Long-term Regulation
Long-term regulation of FAS activity involves modifications in the expression of FAS,
and is highly dependent on the nutritional and hormonal conditions in lipogenic tissues.
Nutritional Regulation of FAS
Nutritional and hormonal stimuli have been shown to regulate FAS transcription.
Carbohydrate fasting and re-feeding, for example, up-regulates FAS expression, and insulin has
been implicated as a possible regulator of this elevation in FAS. Lakhshmanan et al have shown
that feeding a high carbohydrate, fat-free diet to rats fasting for 48-h causes a supraphysiologic increase of hepatic FAS expression and activity compared to normally fed rats [129]. In a follow- up study, they showed that male Holtzman rats – a strain of diabetic rats – do not exhibit the same increase in hepatic FAS activity upon refeeding after a 48-h fast [130]. However, after treatment with insulin, FAS expression in these rats becomes elevated to the supraphysiologic levels observed in the normal “fasting and re-fed” rats. Similarly, insulin has been shown to stimulate an approximately five- and three-fold increase in FAS mRNA and transcription rate in adipocytes and hepatoma cells, respectively; glucagon, on the other hand, suppressed FAS expression in these cells [131]. These results therefore indicate that FAS expression is highly responsive to the dietary insulin response.
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Regulation of FAS in Hormone-Sensitive Tissues
As mentioned above, FAS is also highly expressed in hormone-sensitive cells such as in
the mammary glands. During lactation, stimulation of FASN expression and activity in the
mammary glands are considered to be due to the increases in cortisol, prolactin, and insulin and
the decrease in progestins [132]. Furthermore, during the menstrual cycle, the expression of FAS
in the human endometrium is closely linked to the expression of the proliferation antigen Ki-67,
estrogen receptor, and progesterone receptor, which suggest a functional connection between
FAS and the estradiol (E2)/estrogen receptor–dependent signaling in the normal control of endometrial cell proliferation [133].
1.3.5 - Transcription of FAS
Several transcription factor binding regions have been identified in the FAS promoter
such as the sterol response element (SRE), insulin response element (IRE), carbohydrate
response element (ChRE) and the cAMP response element (CRE). Transcription factors that
have been identified to bind these DNA elements in the FAS promoter and determine the degree
of cellular FAS transcript expression including: sterol response element binding proteins
(SREBP), upstream stimulatory factors (USF), and specificity protein (Sp1) [95,130]. Figure 1.6
illustrates showing the binding areas for these transcription factors in the FAS promoter.
SRE IRE
E-Box (USF) (SREBP) __(Sp1)__ (SREBP) E-Box (USF)
Figure 1.6: The FAS promoter region showing the binding areas for transcription factors involved in the regulation of FAS expression.
33
This section discusses the relationships between these transcription factors and FAS in
normal tissues.
SREBP-1
SREBP-1 belongs to the basic-helix-loop-helix leucine zipper class of transcription
factors. There are two isoforms of SREBP-1, 1a and 1c, both of which are derived from the same gene but through alternative splicing. The major isoform expressed in most cells is SREBP-1a, whereas SREBP-1c is the major isoform in animal liver and adipose tissue [134,135]. SREBP-1
is necessary for lipogenesis stimulation, as SREBP-1 knockout mice have an impaired FAS
response to carbohydrate feeding [136]. In contrast, transgenic mice that overexpress SREBP-1c
in the liver, have an increased level of both FAS mRNA and activity [137]. SREBP-1 has two
potential binding sites on the FAS promoter. One is the sterol response element (SRE) located at
position -150 of the proximal promoter, the other is the E-box motif at position -65, that is the
binding site of USF [138]. However, SREBP-1 binding to the E-box occurs in vitro only, and
studies show that the physiologically relevant site of SREBP-1 binding is the SRE at -150 [139-
141].
USFs
USFs are members of the basic-helix-loop-helix (bHLH) family of transcription factors
that bind to the E-box motif on the FAS promoter [142]. Two forms of USF, USF-1 and USF-2
are encoded by separate genes, and studies have identified that USFs are major components of
the protein complex binding to the insulin response sequence FAS-IRS-A, located at position -65
and at position -332 in the proximal FAS promoter region [143, 144]. USF binding to the E-
boxes is required for insulin regulation of FAS, as mutations within the E-box completely
34
remove the insulin response [143], and USF-1 and USF-2 -/- mice show reduction in FAS transcription after fasting/refeeding [145].
Sp1
Sp1 is a member of family of the Specificity Protein/Kruppel-like transcription factors.
Sp1 is a ubiquitously expressed, sequence-specific DNA-binding transcription factor that activates a broad and diverse spectrum of mammalian and viral genes [88]. Sp1 recognizes
GC/GT boxes in gene promoters and interacts with DNA through three C2H2-type zinc fingers located at the C-terminal domain. Based on results of crystal structure and NMR studies, each of the three zinc fingers in Sp1 recognizes three bases in one strand, and a single base in the complementary strand of the GC-rich elements where the consensus Sp1 binding site located 5’-
(G/T)GGGCGG(G/A)(G/A)(C/T)-3’[146]. Wolf et al have shown that the 5' region of the rat fatty acid synthase (FAS) gene has a high GC content between -900 and +500, implying several binding sites for members of the Sp1 family of transcription factors [147]. Using SL2 and H4IIE cells in conjunction with FAS promoter/luciferase constructs either successively deleted or containing defined deletions, Wolf et el characterized seven GC boxes--GC-I to GC-VII--located between -557 and -83 in the FAS promoter. In vitro DNAse I-footprinting, electrophoretic mobility shift assays, and the yeast one-hybrid system indicated that Sp1 interacts with GC-I to
GC-VII and that each of the GC boxes conferred Sp1-dependent transcription.
Sp1 is required in the expression of several genes; however, the specific physiological function of Sp1 has not been determined [148]. Results of gene knockout studies in mice have provided valuable insight on some of the critical functions of this gene. For example, Marin et al showed that Sp1 -/- embryos exhibit multiple abnormalities and retarded development and embryolthality on day 11 of gestation [149]. Furthermore, Sp1 -/- mice also exhibit defects in
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late tooth formation and death at birth [150,151]. Therefore, Sp1 is a critical factor required for
normal physiolocial development.
1.4 - FAS and Cancer
As mentioned above, FAS is closely regulated by nutritional and hormonal factors and
normally remains at very low levels in normal cells. These tissues sufficiently obtain any
necessary fatty acids from the diet. On the other hand, in 1989, Kuhajda et al identified FAS as a
molecule that was highly expressed in the tumor cells of breast cancer patients [152]. Indeed,
immunohistochemical results of surgical samples have since revealed that FAS is highly
expressed in a number of cancers, including the breast, endometrium, prostate, colon, thyroid
gland, ovaries, stomach and lungs; and that FAS is a prognostic marker of these types of cancer
[153-161]. In all these cases, FAS expression has been found to be significantly higher in the tumor sections of these tissues compared to their surrounding normal tissues. In addition, several rodent studies have shown that chemically or virally induced mammary tumors also overexpress
FAS [162-164]. Similar studies have also shown positive associations between FAS overexpression and cancer aggression [153, 154, 156, 157].
The function of FAS overexpression in cancer, and how it contributes to cancer growth and development remains unclear. However, it is hypothesized that FAS over-expression
contributes to cellular proliferation through adequately supplying membrane lipids, as well as
supplemental energy, via β-oxidation of fatty acids in cancer cells [165]. It has also been
suggested that palmitate and myristate, the major products of FAS, may be required at high
levels in cancer cells for the lipidation of signalling proteins such as G-protein subunits, nonreceptor tyrosine kinases, and Ras proteins [166,167]– all of which are required in cancer- associated pathways.
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For our experiments, we have focussed on FAS expression in breast cancer cells. The
following section will briefly review the current literature on FAS overexpression in breast
cancer.
1.4.1 - FAS and Breast Cancer
In human breast cancer patients, FAS overexpression is associated with poor prognosis
[157, 168, 169]. For example, Alo et al. have shown that FAS overexpression in malignant breast
tumors is associated with a four-fold increase in risk of death [157]. Similarly, Jensen et al. observed a nine-fold increase in risk when FAS expression occurred along with a high proliferative index (>17%) [168]. In addition to the expression of FAS in fully malignant breast
tumors, human breast cancer patients also have elevated serum FAS levels compared to normal
control subjects using a polyclonal-monoclonal sandwich enzyme immunosorbent assay [170].
Furthermore, high levels of FAS have been found in both in situ duct and lobular carcinomas –
both of which are direct precursor lesions to invasive breast cancer [158, 170]. Hence, elevated
FAS expression in the blood and certain breast regions are indicators of breast cancer (and/or
possibly cancers in other regions).
Cell culture and rodent studies involving FAS inhibitors or siRNA indicate that its over- expression may indeed be required for enhancing certain cancer processes such as cellular proliferation and cell cycle progression, while reducing other processes such as apoptosis.
FAS and cell proliferation, cell cycle and tumour growth
Liu et al have shown that inhibition of FAS by triclosan reduces MCF-7 and SKBr3 breast cancer cell viability and growth [171]. Similarly, Pizer et al showed that inhibition of FAS with C75 reduces cell proliferation and causes a profound inhibition of DNA replication and S
37
phase progression of MCF-7 cells [172]. Menendez et al showed that the FAS inhibitor orlistat
reduces cell proliferation of SKBr3 cells, by leading to S-phase cell cycle arrest and by down-
regulating HER2/neu oncogene expression [173] (HER2/neu is a cell membrane-bound receptor
tyrosine kinase, commonly involved in the pathogenesis of breast cancer). Knowles et al showed
that in MDA-MB435 breast cancer cells, ablation of FAS activity with orlistat or siRNA caused a dramatic downregulation of Skp2, a component of an E3 ubiquitin ligase that tags p27Kip1 for
degradation by the proteasome [174] (p27Kip1 is an inhibitor protein that prevents the activation of cyclin E-CDK2 or cyclin D-CDK4 complexes, and thus controls the cell cycle progression at
G1). The reduction in Skp2, in turn, resulted in an upregulation of p27Kip1 and a cell-cycle arrest
at the G1/S boundary, ultimately reducing the proliferation rate of these cells. Furthermore, Lu et
al showed that MNU-induced rats fed diets containing 1000 ppm triclosan have a significant
reduction in the size and incidence of mammary tumors compared to control rats [121].
FAS and apoptosis
Pizer et al report that within 6 h after exposure to cerulenin, ZR-75, SKBr3 and MCF-7
breast cancer cells express lower levels of FAS [175]. Within the same interval, loss of
clonogenic capacity occurs, followed by DNA fragmentation and morphological changes
characteristic of apoptosis. Similar outcomes have also been observed following triclosan
treatment [171].
Moreover, FAS inhibition also sensitizes breast cancer cells to other apoptotic agents.
Menedez et al showed that pharmalogical and siRNA mediated inhibition of FAS synergistically
enhances Taxo (Paclitaxel)-induced apoptosis in MDA-MB-231 and MCF-7 cells [176]. In
MDA-MB-231 cells, FAS inhibition suppresses HER2/neu oncogene overexpression, and synergistically enhances apoptosis by anti-HER2 antibody trastuzumab [177]. Furthermore,
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Kumar-Sinha et al have shown that inhibition of FAS preferentially induces apoptosis in HER2- transfected breast epithelial cells compared to matched vector-transfected control cells [178].
1.4.2 - FAS and Other Cancers
Elevated FAS expression is also a characteristic of other types of cancer. Several studies have evaluated FAS overexpression in colon cancer. Rashid et al used immunohistochemistry to show that FAS was high in essentially all colon cancer samples evaluated, in comparison to their normal surrounding mucosa [159]. FAS has also been shown to be overexpressed in most human colon adenomas [179]. In addition, inhibition of FAS in HCT116 colon cancer cells results in a reduction of their proliferation [180].
A number have studies show that FAS expression is associated with prostate cancer progression [153,154]. Both LNCaP and PC-3 prostate cancer cells have been shown to overexpress FAS. Orlistat inhibits proliferation and induces apoptosis in both of these cell lines
[115]. Furthermore, FAS has also been shown to be elevated in the endometrium, ovaries, stomach, lungs and tongue [156, 160, 161, 181].
1.4.3 - Regulation of FAS in Cancer
The ultimate mechanism responsible for tumor associated FAS expression is not completely understood; however, several hormones and signalling pathways have been shown to be involved in FAS over-expression (all of which are illustrated in Figure 1.7).
At the transcriptional level, growth factors (GFs) and GF receptors (GFRs) have emerged as major contributors to FAS over-expression in tumour cells. For example, FAS expression in breast, prostate and ovarian cancer cell lines has been shown to be stimulated by epidermal growth factor (EGF), and by the EGF receptor (EGFR) [182], which in turn, results in over
39
expression of FAS by activating the phosphatidylinositol-3 kinase (PI3K)–Akt signalling pathway.
EGFs and EGFRs have also been shown to affect FAS expression through the mitogen- activated protein kinase (MAPK) extracellular signal-regulated kinase (ERK1/2) signalling
cascade in tumour cells [182].
Steroid hormones (SHs) including estrogen, progestins and androgens also have an
important role in regulating FAS gene expression and the FAS biosynthetic pathway as part of
the SH-driven cellular response [182]. The regulatory effects of SH on FAS gene expression,
downstream of the SH receptors (SHRs) ER, PR and androgen receptor (AR) also involve
aberrant activation of the PI3K–Akt and ERK1/2 signal transduction pathways [182].
Figure 1.7: Regulation of FAS expression in cancer by growth factors and steroid hormones [image taken from ref 183].
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Post-translational regulation may also contribute to the upregulation of FAS in cancer
cells. In LNCaP prostate cancer cells, FAS has been found to interact with the pre-proteosomal ubiquitin-specific protease USP2a, which removes ubiquitin and strongly stabilizes FAS (Figure
1.8) [182]. Knockdown of USP2a reduces FAS expression, decreases cell proliferation and induces cell death, whereas apoptosis is rescued by FAS overexpression [183]. The relevance of this regulatory mechanism on FAS expression in other tumours, however, is largely unknown.
Figure 1.8: Post-translational regulation of FAS in cancer. Interaction between FAS and USP2a prevents proteasomal degradation of FAS [image taken from ref 183].
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1.4.4 - Transcription Factors Regulating FAS in Cancer
Although several transcription factors contribute to the regulation of expression of FAS in
cance, the existing literature has primarily focused on two in particular: SREBP-1c and Sp1.
SREBP-1c
FAS over-expression in both nutritionally controlled endogenous fatty acid synthesis in
liver and adipose tissue and in cancer occurs through the modulation of the expression of the
transcription factor SREBP-1c. In both cases, hormones stimulate FAS transcription when
SREBP-1c interacts with the SREBP-binding site at the endogenous FAS promoter. Although intracellular signalling cascades that regulate FAS expression in normal and tumour cells seem to share identical downstream elements, including PI3K, MAPK and SREBP1c, the upstream mechanisms controlling FAS expression in cancer cells may be different, as tumour-associated
FAS seems to be insensitive to nutritional signals [182].
In lipogenic cells, the effects of carbohydrates and dietary fatty acids on FAS expression are mainly mediated by hormones, which stimulate (insulin, tri-iodothyronine and glucocorticoids) or inhibit (leptin, glucagon and cyclic AMP) FAS-dependent lipogenesis. In tumour cells, SREBP-1c expression and activation will be driven by aberrant GF and GFR and/or SH and SHR-driven signalling. Supporting this notion, inhibitors of PI3K and MAPK downregulate SREBP1c and decrease FAS transcription, ultimately reducing neoplastic lipogenesis in cultured cancer cells. Furthermore, FAS overexpression by oncogenic stimuli can also be abrogated by deletion of the major SREBP binding site from the FAS promoter. As well,
Akt stimulates the synthesis and nuclear accumulation of activated SREBP1c [182].
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Sp1
Sp1 is over-expressed in a variety of cancers including breast cancer, and plays an important role in cell growth regulation by modulating the expression of several cell cycle regulatory proteins [148]. As mentioned above, Sp1 regulates gene expression by binding to
‘Sp1 sites’ that include GC-boxes. The promoters of the genes encoding two enzymes of fatty acid synthesis, ACL and ACC, are known to contain Sp1 sites [182], and recently, we have shown that FAS over-expression in cancer cells is also regulated by Sp1. Using the estrogen- responsive MCF-7 human breast cancer cell line, Lu et al [184] demonstrated by RNA interference and ChIP analysis that Sp1 plays a role in regulating FAS expression at the FAS promoter level. Interferce of Sp1 binding at the FAS promoter resulted in a reduced expression on FAS and reduced cell proliferation. Similarly, blocking Sp1 binding sites with the drug mithramycin, also caused a decrease in FAS expression and proliferation. Conversely, 17β- estradiol, a stimulator of MCF-7 proliferation, increased binding of Sp1 to the FAS promoter, increased FAS expression and increased cell proliferation; suggesting that the transcription factor
Sp1 is a molecular link between de novo lipogenesis and proliferation in breast cancer cells
[184]. The next and final section of this chapter briefly reviews the existing studies of Sp1 in cancer.
1.4.5 -Sp1 and Cancer
Sp1 has been shown to be elevated in a number of cancers. Zanetti et al [185] showed that Sp1 was elevated in the breast carcinomas of 11 out of 14 patients, whereas only 1 of 5 benign breast lesions expressed detectable levels of Sp1. Chiefari et al [186] showed that Sp1 was over-expressed in thyroid tumours compared to normal tissues, whereas, Shi et al [187] showed that Sp1 is over-expressed in pancreatic tumours compared to normal tissues. Hosoi et al
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[188] have shown that DNA-dependent protein kinases Ku70 and Ku80 are upregulated in colon
tumours compared to normal and adjacent tissues. Sp1 is known to regulate these genes and was
also shown to be elevated in these tumours. A promoter analysis confirmed that constitutive
expression of these kinases was due to the increased interaction of Sp1 with the GC-rich regions
in the promoters of these genes [188].
There is a significant amount of evidence indicating that Sp1 over-expression is a critical
factor in the regulation of several cancer cell processes, specifically the expression of genes
involved in cell cycle progression, angiogenesis, apoptosis and metastasis.
Cell Cycle Progression
In various cancer cell lines, Sp1 has been shown to play an important role in sustaining
cell cycle progression. For example, inhibition of Sp1 suppressed cell growth and caused G1
phase arrest in human glioblastoma, lung and pancreatic cancer cells [189, 190]. A dominant- negative Sp1 mutation in Hela cells decreased cell growth, led to G1 phase arrest, reduced expression of cyclin D1 and increased expression of p27 [191]. Another study in Hela cells showed that ectopic expression of dominant negative Sp1 reduced growth rate by prolonging the
S phase [192]. As well, in serum-starved MCF-7 cells, Abdelrahim et al showed that Sp1 siRNA transfection blocked estrogen-stimulated cell cycle progression by causing G1 phase arrest [193].
Angiogenesis
Vascular endothelial growth factor (VEGF), a growth factor involved in angiogenesis, has been shown to be regulated by Sp1 in various cancers [189,190]. Wang et al [194] showed that Sp1 was highly expressed in nuclei of gastric tumour cells, whereas minimal to non- detectable levels were detected in stromal or normal glandular cells within or surrounding the
44
tumours. They also showed that the survival of patients with high Sp1 expression was
significantly decreased compared to patients with weak to non-detectable Sp1 expression.
Similarly, Shi et al showed that Sp1 as over-expression in pancreatic tumour cell lines correlates with elevated VEGF levels [187].
Apoptosis and Metastsis
Resistance to apoptosis has been associated with over-expression of Sp1 in cancer cells.
Sp1 sites have been located in the promoters of the anti-apoptotic genes Bcl-2, Bcl-3, Bcl-x, survivin and Bak [195]. Sp1 sites have also been located in the promoter regions of the matrix metalloproteinase-2 (MMP-2), a gene associated with metastasis in cancer. Bae et al [196] investigated invasiveness of SNU-484 and SNU-638 gastric adenocarcinoma cell lines. They showed that Bcl-w and Bcl-2 were overexpressed in both cell lines, and this was associated with their migratory and invasive potentials. Blocking Sp1 using pharmacologic inhibitors, dominant- negative mutants, or small interfering RNA reduced Bcl-w and Bcl-2 expression and increased cell apoptosis. Furthermore, blocking Sp1 also reduced MMP-2 expression and reduced cell invasion. Overall, their results suggest that Sp1 overexpression in cancer may be necessary for cell survivability and invasiveness.
1.5 Research Hypothesis and Objectives
As described above, in contrast to normal cells, most cancer cells over-express the
enzyme FAS to provide lipids for membrane production to support a high rate of proliferation
[152]. This differential degree of FAS expression between normal and cancer cells make FAS an
ideal target for cancer prevention.
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Sp1 binding sites exist in regions of the FAS gene promoter [148] and previous findings in our lab suggest that Sp1 regulates the expression of FAS in MCF-7 breast cancer cells [182].
More specifically, we showed that binding of Sp1 at the FAS promoter coordinately regulates
FAS over-expression and proliferation in MCF-7 cells.
While drugs that inhibit FAS (e.g. cerulenin and orlistat) effectively inhibit cancer cell proliferation, they produce undesirable side effects [110, 113, 117, 121]. Dietary compounds, on the other hand, that are capable of inhibiting FAS are being sought as an alternative to these drugs. Two possible compounds include the dietary indoles I3C and DIM, which have been shown to reduce cancer cell proliferation and modify the expression of Sp1-regulated enzymes in cancer cells.
Therefore, the objective of our study was to determine if the I3C or DIM-induced reduction of MCF-7 growth was caused by a reduction in FAS expression. Since both compounds have been shown to reduce expression of Sp1-associated cancer genes, we hypothesized that I3C and DIM will reduce MCF-7 proliferation and will also reduce FAS expression.
Furthermore, we also chose to analyze the effect these indole compounds have on breast cancer cells that express FAS at levels that differ from that of MCF-7 cells. Menendez et al [165] have shown that MCF-7 cells have a moderate level of FAS over-expression, whereas comparatively, MDA-MB-231 cells have a low FAS expression level, while SKBR-3 cells have a very high FAS over-expression level (indeed, 28% of total soluble proteins expressed in
SKBR-3 cells is FAS [165]). Therefore, the specific objectives of our study were to determine 1) if I3C or DIM affect the proliferation and FAS expression of three different breast cancer cells lines and one normal mammary tissue line 2) if the I3C or DIM-induced reduction of cell growth can be reversed by fatty acid supplementation and 3) if Sp1 is affected by I3C or DIM.
CHAPTER TWO:
MATERIALS AND METHODS
46
47
2.1 – Cell Culture Conditions
MCF-7, MDA-MB-231, SKBr3 and MCF-10A cell lines were purchased from the
American Type Cell Culture collection and routinely maintained in T-75 flasks (75 cm2 area) and
subcultured every 5-7 days (~80-90% confluency) with medium renewal every 1-2 days. Cells of
4-7 passage generations were used for all experiments. All cell culture reagents were obtained
from Gibco-Invitrogen (Burlington, ON, Canada) and cell culture materials were obtained from
BD Biosciences (Missisauga, ON, Canada) except where noted. MCF-7 and MCF-10A cells were cultured in high glucose Dulbecco’s Modified Eagle Medium (DMEM) F12, SKBr-3 in
McCoy’s 5A medium, and MDA-MB-231 in Iscove’s Modified Dulbecco’s Medium (IMDM).
All media contained 1% penicillin/streptomycin and were supplemented with 10% fetal bovine
serum (FBS, Sigma-Aldrich Canada Ltd., Oakville, ON, Canada).
o Cells were maintained at 37 C in a humidified atmosphere of 95% air and 5% CO2. As
well, cells were screened periodically for contamination.
2.2 - Cell Treatment
Indole-3-carbinol (I3C) was obtained from Sigma-Aldrich Canada Ltd and 3,3’-diindolyl- methane (DIM) from Designed Nutritional Products (Orem, Utah, USA). Stock solutions of 200 mM I3C and 100 mM DIM were prepared by dissolving each indole compound in dimethyl
sulphoxide (DMSO) (Hybri-max®, Sigma-Aldrich Canada Ltd.). Stock solutions were stored at
−20 °C in the dark prior to use. Final concentrations were made such that diluting the I3C or
DIM stock into media would result in an initial concentration of 100 μM I3C or 50 μM DIM (or
none in control), 10% FBS (v/v) and 0.05% DMSO (v/v).
The half-life of I3C in medium is approximately 40 hours, while that of DIM is
approximately 35 h; hence, the medium was changed once a day for a total of 72 h for I3C
48
treated cells and 48 h for DIM treated cells. These incubation durations are commonly used in studies testing the effects of I3C or DIM in culture.
2.3 - Cell Proliferation Analysis
Cell proliferation was determined using a standard colorimetric MTT (3-4, 5-
dimethylthiazol-2-yl-2,5-diphenyl-tetrazolium bromide) assay. MTT is converted from a yellow-
coloured tetrazolium salt to a purple-coloured formazan in the cells by cleavage of the
tetrazolium ring by mitrochondrial dehydrogenases, the activity of which is linear to the cell
number.
Briefly, cells were plated at a density of 5x104/100μl/well in 96-well microtitre plates and allowed an overnight period for attachment. Then the medium was removed and fresh medium alone (control) or fresh medium final concentrations of 100 μM I3C or 50 μM for DIM were
added to cultures in parallel.
Following this treatment, cells were treated with phenol-red-free DMEM medium
containing 5% MTT (that is, the medium did not contain FBS, I3C or DIM). The cells were
incubated with the MTT dye for 4 hours at 37oC. After removing the supernatants, the MTT-
formazan crystals were dissolved with a solution of 0.4N HCl in isopropanol (100μl/well) and
the absorbance was measured at 570 nm in a multi-well plate reader (Bio-Rad Microplate
Reader, Model 550).
2.4 - Preparation of Whole Cell Extracts and Western Blot Analysis
Cells were washed with ice-cold phosphate-buffered saline then incubated with cold lysis buffer (50mM Tris-HCl, pH 7.5, 1 mM EDTA, 1mM EGTA, 0.5 mM Na3VO4, 10 mM
glycerophosphate, 5 mM NaF, 1 mM phenylmethylsulfonyl fluoride, and 40 µg/ml each of
pepstatin A, aprotinin, and leupeptin) for 30 min, and centrifuged at 16,000 x g for 15 min.
49
Supernatants were stored at -80ºC for Western blot analysis. Due to their varying level of FAS protein, for MCF-7, MDA-MB-231, SKBr-3 and MCf-10A cells, 5, 5, 1 and 12ug of protein was injected into each western gel well, respectively.
The proteins from whole cell extracts were separated by 10% SDS-PAGE, and were transferred onto PVDF membranes (Bio-Rad Laboratories, Inc., Hercules, CA) using a semi-dry blotter (C.B.S. Scientific Co., Del Mar, CA). Membranes were blocked with 5% non-fat dried milk in TTBS (10 mM Tris-HCl, pH 8.0, 100 mM Nacl, and 0.05% Tween 20) for 1 h at room temperature, then incubated overnight at 4ºC with either mouse monoclonal anti-human FAS antibody at 1:1000 dilution (BD Transduction Laboratories, Missisauga, Ontario, Canada) or mouse monoclonal anti-human Sp1 antibody (Santa Cruz Biotechnology, Inc.) at 1:5000 dilution for 45 min at room temperature. Bands were visualized on Kodak X-ray imaging film, which was developed using a Kodak M35A X-OMAT Processor (Toronto, ONT).
Membranes were stripped in 62.5 mM Tris pH 6.7, 100 mM β-mercaptoethanol and 2%
SDS, for 30 min at 50ºC.β -actin was used as a loading control. Bands were quantified using a
FluorChem digital imager (Alpha Innotech Corp, San Leandro, CA, USA).
2.5 - Preparation of Total RNA
Total RNA was isolated from MCF-7 cells using TRI REAGENTTM (Sigma-Aldrich
Canada Ltd.) according to the manufacturer’s protocol for cell culture RNA preparation. Briefly,
3 ml of medium containing cells were plated in 100x20mm culture dishes at a cell density of
5x105/ml. Cells were allowed one day to attach and grow to approximately 30% confluency.
Next, cells were treated with FBS containing medium only or with medium containing DIM (and
FBS) for 2 days. The medium was then removed and 1 ml of TRI REAGENTTM was applied to the cell monolayer. The lysate was then collected, mixed with isopropanol (0.5ml), allowed to stand for 10 minutes, and centrifuged at 12,000g for an additional 10 minutes at 4ºC. The
50
supernatant was removed and the RNA pellet was washed by adding 1ml of 75% ethanol,
vortexing and centrifuging for 5 minutes at 4ºC. The RNA pellet was then air-dried for 5-10
minutes, dissolved in RNase-free dH2O and stored at -80ºC. RNA concentrations were measured
at 260 and 280 nm to ensure a ratio of >1.7, indicating the RNA is free of proteins and DNA.
2.6 - Preparation of cDNA and Real-time PCR Analysis
First Strand cDNA Synthesis KitTM by Fermentas (Burlington, ONT) was used to prepare
cDNA for real-time PCR according to the manufacturers instructions. Two µg of total RNA, 2µl
of primer, 12 µl of DEPC-treated water, 8 µl of 5x reaction buffer, 2 µl of RiboLock RNase
inhibitor 4 µl of 10mM dNTP and 4 µl of reverse transcriptase were mixed and incubated for 60
minutes at 37ºC. Heating the tubes to 70ºC for 5 minutes terminated the reaction.
All real-time PCR analysis was done using an ABI Prism 7000 Sequence Detection
System (Applied Biosystems, USA). Sp1 and β-actin primers and probes were purchased from
Applied Biosystems (Foster City, CA, USA). Each PCR-reaction was performed in triplicate on
a 96-well PCR plate, and each reaction well contained 1 µl of cDNA products, 1 µl of either Sp1
or β-actin primers and probes, 8 µl of distilled water, and 10 µl of Taqman® Universal PCR
Master Mix (Applied Biosystems, USA). Two amplification efficiency tests were performed,
using cDNA samples prepared from two different experiments, to calibrate the system and
confirm that β-actin was indeed a suitable control gene for this experiment.
Quantification of Sp1 expression was accomplished by measuring the fractional cycle
number at which the amount of expression reached a fixed threshold (CT). The relative
quantification was given by the average CT values (from the triplicates) for Sp1 and β-actin. CT
values were averaged and the Sp1 CT value was subtracted from the β-actin CT to obtain ΔCT. The
-ΔΔCT relative expression level of Sp1 was determined as 2 where ΔΔCT represents ΔCT from DIM
treated cells minus ΔCT from untreated cells.
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2.7 - Rescue Experiments
Palmitic acid and oleic acid were obtained from Sigma-Aldrich Canada Ltd. Stock
solutions of 60 mM of each fatty acid were prepared by dissolving palmitic acid in DMSO and
oleic acid in ethanol. Stock solutions were protected from light with aluminum foil and stored at
−20 °C in the dark prior to use.
MCF-7 cells were plated at a density of 5x104/100μl/well in 96-well microtitre plates in
DMEM-F12 medium containing 10% FBS and 1% BSA (BSA, fraction V, Sigma-Aldrich
Canada Ltd.) and allowed an overnight period for attachment. For these experiments, medium
containing BSA was always prepared fresh before fatty acid stock solutions were diluted in it.
Rescue with palmitate
Cells were treated with medium alone, medium containing 20 µM palmitic acid, medium
containing 50 μM for DIM, or medium containing 20 µM palmitic acid and 50 µM DIM, for
48h. Testing was also performed with 30 µM palmitic acid and 25 µM DIM. The total
concentration of DMSO in the medium was kept contant between treatments.
Rescue with oleate
Cells were treated with medium alone, medium containing 7.5-30 µM oleic acid alone,
medium containing 50 µM DIM alone or with medium containing 7.5-30 µM oleic acid and 50
µM DIM, for 48h. The total concentration of ethanol and DMSO in the medium was kept contant
between treatments.
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2.8 - Inhibition of FAS with Cerulenin
Cerulenin was purchased from Sigma-Aldrich Canada Ltd. A stock solution of 10mg/ml was prepared by dissolving the compound in DMSO. The stock solution was protected from light with aluminum foil and stored at −20 °C in the dark prior to use.
MCF-7 cells were treated with a final concentration 5-10 μg/ml of cerulenin as positive controls during the palmitate and oleate rescue experiments (described above). The effect of 10
μg/ml cerulenin on MCF-10A was also tested. In all cases, the total concentration of DMSO in the medium was kept contant between treatments.
2.9 - Statistical Analysis
All statistical analyses were performed using GraphPad Prism 4.0 software (GraphPad,
San Diego, CA, USA). Student’s t-tests were used to compare two means, while comparisons of multiple means were analyzed with a one-way ANOVA (with Tukey’s post-hoc tests). All values were expressed as means +/- SEM. For proliferation figures, means were derived from 24 similar repetitions. For western blot densitometry figures, means were derived from 3 separate repetitions.
CHAPTER THREE:
RESULTS
53
54
3.1 - The Effect of I3C on MCF-7 Cells
I3C inhibits proliferation
Several studies have measured the effect of I3C on cell proliferation, with incubation times ranging between 2 and 96 h [78-92]. We chose to use an incubation time of 72 h, which is based the I3C exposure durations used in MCF-7 cell studies by Firestone et al [89-92]. In addition, we tested the effects of I3C on MCF-7 cell proliferation at 48 h, since several cancer- associated proteins in MCF-7 cells have also been shown to be affected by I3C after this exposure duration.
There were significantly fewer cells in wells treated with 100 μM I3C. As shown in
Figure 3.1, I3C added to the culture medium significantly inhibited MCF-7 proliferation after 48 h of incubation by 32% compared to untreated cells. After 72 h, I3C inhibited cell proliferation by 47% compared to untreated cells.
I3C does not alter FAS expression
To determine if the effect of I3C on cell proliferation was associated with changes in
FAS protein expression, we performed Western Blot analysis on extracts of MCF-7 cells grown in the presence of 100 uM I3C. As shown in Figure 3.2, FAS was not significantly affected by
I3C after 48 or 72 h.
55
100 100 * * 80 80 60 60
40 40 PercentControl (%) of PercentControl (%) of PercentControl (%) of PercentControl (%) of 20 20
0 0 Control I3C Control I3C
Figure 3.1: The effect of I3C on MCF-7 proliferation after 48 h (left panel) and 72 h (right panel). All cells were treated with 100 μM I3C. Values are means ± SEM. (*) indicates a significant difference in mean value compared to untreated cells (p<0.01).
100 100
80 80
60 60
40 40 PercentControl (%) of PercentControl (%) of PercentControl (%) of PercentControl (%) of 20 20
0 0 Control I3C Control I3C
FAS FAS
β-actin β-actin
Figure 3.2: The effect of I3C on FAS expression in MCF-7 cells after 48 h (left panel) and 72 h (right panel). Cells were treated with 100 μM I3C. Values are means ± SEM. The actual blots used to generate the above quantivative representations are shown below. In all cases, representative blots of samples from three independent experiments are shown, with β-actin as a loading control.
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3.2 - The Effect of DIM on MCF-7 Cells
DIM inhibits proliferation and FAS expression
Firestone et al [89-92] have shown that DIM has inhibitory effects on MCF-7 cell
proliferation similar to I3C. We tested the effect 50 uM DIM on MCF-7 proliferation for a 48 h incubation duration. In confirmation of the results from the literature, 50 uM DIM reduced the
MCF-7 proliferation by 49% (Figure 3.3). However, unlike with I3C, DIM treatment resulted in a 78% reduction in FAS expression.
48-h time-course of effect of DIM on MCF-7 proliferation and FAS expression
Since DIM reduced both cell proliferation and FAS expression, we further explored this
relationship by performing a time course experiment over the 48 h period. Furthermore, we also
determined if and when Sp1 protein expression was affected in MCF-7 cells treated with DIM.
As shown in Figure 3.4a, DIM significantly inhibited MCF-7 cell growth as early as 12 h
after the treatment application. However, after 12 h, FAS expression in DIM-treated cells was not significantly reduced (Figure 3.4b). There was inhibition of both proliferation and FAS expression at 24 h- 48 h.
Re-probing the same membranes with an anti-body for Sp1, showed a 84% reduction in
Sp1 expression due to DIM treatment at 24 h. At 36 and 48 h, there appeared to be little to no expression of Sp1.
57
100
80 *
60
40
PercentControl (%) of 20
0 Control DIM
100
80
60 *
40
PercentPercentControlControl (%) (%) of of 20
0 Control DIM
FAS
β-actin
Figure 3.3: The effect of DIM on MCF-7 proliferation (upper panel) and on FAS expression (lower panel). Cells were treated with 50μM DIM. Values are means ± SEM. For FAS expression, quantitative representations are shown above, and the actual blots are shown below, with β-actin as the loading control. (*) indicates a significant difference in mean value compared to untreated cells (p<0.01).
58
12h 24h 36h 48h
(a) 100 * * * *
80
60
40 Percent of Control (%) Control of Percent Percent of Control (%) Control of Percent 20
0 Ctrl DIM Ctrl DIM Ctrl DIM Ctrl DIM
(b) 100 * * *
80
60
40
20 Percent of Control (%) Control of Percent (%) Control of Percent 0 Ctrl DIM Ctrl DIM Ctrl DIM Ctrl DIM
(c) 100 * * * 80
60
40
20 Percent of Control (%) Control of Percent Percent of Control (%) Control of Percent
0 Ctrl DIM Ctrl DIM Ctrl DIM Ctrl DIM FAS
Sp1
β-actin
Figure 3.4 – 48 h Time-course evaluation of DIM on MCF-7 (a) proliferation, (b) FAS and (c) Sp1 expression. Cells were treated with 50μM DIM. Values are means ± SEM. (*) indicates a significant difference in mean value compared to untreated cells (P<0.01). For FAS and Sp1 expression, the actual western blots are shown below, with β-actin as the loading control.
59
DIM does not affect Sp1 transcript level
As mentioned in Chapter 1, Sp1 is known to regulate FAS expression in MCF-7 cells
[184]. Since we observed that Sp1 protein was reduced in MCF-7 cells after DIM treatment, we
next determined whether this observed reduction was due to a reduction of Sp1 transcript. Real- time PCR analysis indicated, however, that Sp1 transcript levels were unchanged after 48-hours in DIM treated cells in comparison to untreated cells (data not shown).
3.3 - The Effect of I3C and DIM on MDA-MB-231 Cells
Both compounds inhibit proliferation and FAS and Sp1
Although nearly all cancer cell-lines over-express FAS in comparison to their
untransformed normal counterparts, the degree of FAS over-expression varies between cell lines
[165]. For example, MDA-MB-231 cells have been shown to have a lower FAS expression than
MCF-7 cells. Hence, we determined whether I3C or DIM affect proliferation and FAS expression of MDA-MB-231 cells.
As shown in Figure 3.5a, 100 µM I3C or 50 µM DIM resulted in a 24% and 26%
inhibition of MDA-MB-231 proliferation, respectively. In addition, cells treated with I3C had a
38% and 57% reduction in FAS and Sp1 expression, respectively (Figure 3.5b), while DIM
treatment caused 56% and 73% reductions in FAS and Sp1 (Figure 3.5c).
60
(a) (a)
100 100 * * 80 80 60 60
40 40
Percent of (%) Control Percent Percent of (%) Control Percent Percent of (%) Control Percent Percent of of (%) (%) Control Control Percent Percent 20 20 0 0 Control I3C Control DIM
(b) (b) FAS Sp1 FAS Sp1
100 100 * * * * 80 80
60 60
40 40
Percent of (%) Control Percent Percent of (%) Control Percent Percent of (%) Control Percent Percent of (%) Control Percent 20 20
0 0 Control I3C Control I3C Control DIM Control DIM
(c) Control I3C (c) Control DIM
FAS FAS
Sp1 Sp1
β-actin β-actin
Figure 3.5 - The effect of I3C (left panel) and DIM (right panel) on MDA-MB-231 (a) proliferation and (b) FAS and Sp1 expression. Cells were treated with 100μM I3C for 72h or 50μM DIM for 48h. Values are means ± SEM. (*) indicates a significant difference in mean value compared to untreated cells (P<0.01). For FAS and Sp1 expression, the actual western blots are shown below (c), with β-actin as the loading control.
61
3.4 -The Effect of I3C and DIM on SKBR-3 Cells
Both compounds inhibit proliferation and FAS, only DIM inhibits Sp1
Approximately a third of the total soluble protein in SKBr-3 cells is FAS [165]. As shown
in Figure 3.6, treatment of these cells with 100 µM I3C or 50 μM DIM resulted in an inhibition of cell proliferation by 26% and 45%, respectively. Furthermore, I3C and DIM treatment resulted in FAS expression reductions of 66% and 73% compared to untreated cells. In addition, DIM treatment resulted in a 13% reduction of Sp1 expression. However, I3C did not affect Sp1 expression in this cell line.
3.5 - MCF-7 Proliferation Restoration Experiments
Palmitate does not restore MCF-7 growth
To test whether the downregulation of FAS by DIM in MCF-7 cells caused the inhibition
of proliferation, we next attempted to restore proliferation with palmitate.
Figure 3.7a shows that 20 μM palmitate added MCF-7 cells grown in the presence of
50uM DIM for 48 hours did not restore cell growth. Furthermore, increasing the concentration of
palmitate to 30uM and reducing the concentration of DIM to 25uM did not restore the amount of
cell growth compared to cells treated with DIM alone (Figure 3.7b). Addition of 20 or 30uM of
palmitate to cells in the absence of DIM had no effect on proliferation.
62
(a) (a)
100 100 * *
80 80
60 60
40 40 Percent of Control (%) Control of Percent Percent of Control (%) Control of Percent 20 20 0 0 Control I3C Control DIM
(b) (b)
FAS Sp1 FAS Sp1
100 100 * * *
80 80
60 60
40 40
(%) Control of Percent Percent of Control (%) Control of Percent 20 20
0 0 Control I3C Control I3C Control DIM Control DIM
(c) Control I3C (c) Control DIM
FAS FAS Sp1 Sp1 β-actin β-actin
Figure 3.6 - The effect of I3C (left panel) and DIM (right panel) on SKBr-3 (a) proliferation and (b) FAS and Sp1 expression. Cells were treated with 100μM I3C for 72h or 50μM DIM for 48h. Values are means ± SEM. (*) indicates a significant difference in mean value compared to untreated cells (P<0.01). For FAS and Sp1 expression, the actual western blots are shown below (c), with β-actin as the loading control.
63
(a) (b)
125 125 a a 100 100
a a 75 75
50 50
25 25 Percent of Control of Percent (%) Percent of Control of Percent (%) 0 0
DIM DIM Control Control Palmitate Palmitate + Palmitate + Palmitate
(c)
125
100
a b c d 75
50
Control of Percent (%)
25
0
OA DIM OA uM Control 30uM OA 15uM OA 7.5uM OA + 30uM OA + 15 uM 7.5
Figure 3.7 – Attempted rescue of DIM-treated MCF-7 cells with palmitate (a) and (b) and with oleic acid (c). Treated cells in (a) were incubated with 20μM palmitate, 50 μM DIM or both. Treated cells in (b) were incubated with 30μM palmitate, 25 μM DIM or both. Treated cells in (c) were incubated with 7.5- 30μM oleic acid (OA), 25 μM DIM or combinations of 25 μM DIM and 7.5-30μM OA. Values are means ± SEM. One-way ANOVA determined differences between means. Different letters indicate means that are significantly different from one another (P<0.01).
64
Oleate does not restore MCF-7 growth
Menendez et al [165] have shown that the addition of oleate to the medium of FAS-
inhibited cells is an effective means of restoring cell growth.
Addition of 7.5-30uM oleic acid MCF-7 cells grown in the absence of DIM had no effect
on proliferation (Figure 3.7c). However, in the presence of 50uM DIM, increasing the final
concentration of oleic acid from 7.5 to 30uM progressively decreased cell growth. Furthermore,
7.5-30 μM oleic acid did not restore cells treated with the FAS inhibitor cerulenin after 48 hours;
in contrast, it progressively reduced cell growth compared to cells cultured in the absence of
cerulenin.
3.6 – The Effect of DIM on MCF-10A cells
DIM does not affect MCF-10A proliferation, FAS or Sp1 expression
Unlike the breast cancer cell lines, MCF-10A cells have the characteristics of normal breast epithelial cells in that they are non-tumorigenic and grow in a culture controlled by
hormones and growth factors [197]. Although the effects of I3C and DIM on various cancer cell
lines are well established, the effect of these indoles on the proliferation of this cell lines have
not been reported.
Since it appeared as though there was a stronger anti-proliferative effect with DIM on the three breast cancer cell lines than there was with I3C, we next only tested the effect of DIM
MCF-10A cells. As shown in Figure 3.8 50 µM DIM did not affect MCF-10A cell proliferation after 48 and 72 h incubation periods. Furthermore, DIM treatment did not alter FAS or Sp1 expression of MCF-10A cells after 48 h compared to untreated cells.
65
a)
100
80
60
40 Percent of Control (%) Control of Percent
20
0 Control DIM
b) FAS Sp1
100
80
60
40
Percent of Control (%) Control of Percent 20
0 Control DIM Control DIM
c)
FAS Sp1 β-actin
Figure 3.8 - The effect of DIM on MCF-10A (a) proliferation and (b) FAS and Sp1 expression. Cells were treated with 50μM DIM for 48 h. Values are means ± SEM. For FAS and Sp1 expression, the actual western blots are shown below (c), with β-actin as the loading control.
66
3.7 – The Effect of Cerulenin on MCF-7 and MCF-10A Proliferation
Cerulenin inhibits MCF-7 cell proliferation but does not affect MCF-10A cells.
Cerulenin is a known synthetic inhibitor of FAS activity [104]. Several studies have
shown that cerulenin reduces breast cancer cell proliferation and increases apoptosis [106-109].
In confirmation of the results in the literature, 10 μg/ml cerulenin reduced the MCF-7
proliferation by 69% after 48 h (Figure 3.9a). However, Figure 3.9b shows that the same
concentration of cerulenin does not affect MCF-10A growth, even after 72 h.
67
(a)
100
80 *
60
40 Percent of Control (%) Control of Percent
20
0 Control Cerulenin
(b) 100
80
60
40 (%) Control of Percent 20
0 Control Cerulenin
Figure 3.9 - The effect of cerulenin on (a) MCF-7 and (b) MCF-10A proliferation. MCF-7 and 10A cells were treated with 10μg/ml cerulenin for 48 and 72 h, respectively. Values are means ± SEM. (*) indicates a significant difference in mean value compared to untreated cells (P<0.01).
CHAPTER FOUR:
GENERAL DISCUSSION AND CONCLUSION
68
69
4.1 - Discussion
Both I3C and DIM have been shown by others to suppress the proliferation of various
cancer cell lines including those of breast [77-94], colon [198-200], prostate [201-204], lung
[205] and endometrium [206, 207]. Our first task was to attempt to reproduce the antiproliferative effect of these compounds on MCF-7 cells in our hands. Concentrations of 10-
150 µM I3C and 1-100 µM DIM have been shown to reversibly inhibit MCF-7 proliferation. As discussed in Chapter 1, concentrations of up to 150 µM for I3C and 50 µM for DIM are relevant to humans. I3C and DIM must be taken as a supplement, however, to achieve a comparable serum concentration, since dietary intake of glucobrassicin, the precursor of I3C in cruciferous vegetables, is much lower [52-55]. The doses and exposure durations for our experiments were based on those established in studies on MCF-7 cells by the Bjeldanes and Firstone group [89-
92], who have demonstrated strong antiproliferative effects with concentrations of 100 µM for
I3C and 50µM for DIM, and exposure times of 72 and 48h, respectively. For example, Cram et al [89] and Cover et al [91] showed an 80% reduction in proliferation after 72 h treatment with
100 µM I3C, while Chang et al [90] and Hong et al [66] showed that 48 h treatment with 50 µM
DIM caused an approximately 55% reduction in proliferation. Under similar, though not identical conditions, we showed that I3C and DIM suppressed growth of MCF-7 cells by 47 and
49%, respectively (Figures 3.1 and 3.3).
Our next objective was to determine whether I3C and DIM have a similar anti- proliferative effect on breast cancer cell lines that have lower and higher amounts of FAS expression compared to MCF-7 cells. For MDA-MB-231 cells, Cover et al [91] showed that 100
µM I3C caused a 31% reduction of proliferation after 72 h, while Moiseeva et al [208] showed that 50 µM DIM caused a reduction of 19% after 48 h. Consistent these findings, we showed that
100 µM I3C suppressed MDA-MB-231 growth by 24 % after 72 h (Figure 3.5a), while 50 µM
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DIM suppressed MDA-MB-231 growth by 26% after 48 h. Furthermore, we showed that 100
µM I3C reduced proliferation of a third breast cancer line, SKBr-3 by 26% after 72 h, while 50
µM DIM reduced SKBr-3 proliferation by 45% after 48 h (Figure 3.6a). To our knowledge, no previous studies have shown these indole compounds to reduce SKBr-3 proliferation. Hence, I3C and DIM suppress the growth of breast cancer cell growth in culture to similar extents, regardless of their degree of FAS over-expression. Tables 4.1 and 4.2 summarize our results for the effect that I3C and DIM had on proliferation, FAS and Sp1 expression on all cell lines tested.
MCF-7 MDA-MB-231 SKBr-3
Proliferation ↓ ↓ ↓
FAS No change ↓ ↓
Sp1 Not measured ↓ No Change
Table 4.1 – The effect of I3C on proliferation, FAS and Sp1 expression in MCF-7, MDA-MB- 231 and SKBr-3 cells.
MCF-7 MDA-MB-231 SKBr-3 MCF-10A
Proliferation ↓ ↓ ↓ No Change
FAS ↓ ↓ ↓ No Change
Sp1 ↓ ↓ ↓ No Change
Table 4.2 – The effect of DIM on proliferation, FAS and Sp1 expression in MCF-7, MDA-MB- 231, SKBr-3 and MCF-10A cells.
71
Using the same number of doubling times we had for the cancer cell lines, we next tested whether DIM would affect the growth of the non-tumorigenic mammary epithelial cell line,
MCF-10A. For these experiments we selected to test only the effect DIM had on proliferation, since we had already shown that DIM causes a greater reduction of MCF-7 proliferation than
I3C. Interestingly, we found that DIM did not affect MCF-10A cell growth (Figure 3.8a). This novel observation suggests that the inhibitory effect of DIM may be specific to cancer versus non-cancer cells. Rahman’s labratory have shown that this effect may also be true for I3C [209].
They investigated the effect I3C has on MCF-10A cells in comparison to the tumorigenic breast epithelial cell line MCF-10CA1a (CA1a), and showed that CA1a cells are more sensitive to growth inhibition by 50 µM than MCF-10A cells. These results, along with ours for DIM, indicate that both I3C and DIM do not affect on normal breast cell growth. Since we have shown that both I3C and DIM reduce proliferation of three breast cancer cell lines, we suggest that these indole compounds may be targeting genes important to cancer cell proliferation, but not to normal cell growth.
Kuhajda et al were the first to show that FAS is highly expressed in tumor cells of breast cancer patients [152]. Since then, FAS has been shown to be highly expressed in a number of cancers, including the breast, endometrium, prostate, colon, thyroid gland, ovaries, stomach and lungs [153-164]. It is thought that FAS is over-expressed in cancer tissues for membrane synthesis to sustain an elevated rate of cell division. Hence, we were interested in understanding if the anti-proliferative effect of I3C and DIM involves a modification of FAS expression. The rational behind this idea was that both I3C and DIM have been shown to modify the expression of certain genes in MCF-7 cells requiring the transcription factor Sp1[89, 92] and the FAS gene promoter includes binding sites for Sp1 [184].
72
Since all three breast cancer cell lines over-express FAS, we expected I3C would reduce the expression of this enzyme in all of them. Our results, however, indicate that I3C and DIM have varying effects on FAS expression, and suggest that the two compounds may be acting to reduce proliferation possibly through different mechanisms. Although I3C caused a reduction in the proliferation of all three breast cancer cell lines, it caused a downregulation of FAS in MDA-
MB-231 cells and SKBr-3 cells (Figures 3.5b and 3.6b) but did not significantly reduce expression of FAS in MCF-7 cells (Figure 3.2). As mentioned above, compared to MCF-7 cells,
SKBr-3 and MDA-MB-231 cells have a relatively higher and lower amounts of FAS, respectively. Thus, these results suggest that the inhibitory effect of I3C on cell proliferation is not caused by a downregulation of FAS.
On the other hand, the reduction in breast cancer cell proliferation we observed after treatment with DIM was associated with a reduction in FAS expression in all three cancer cell lines (Figures 3.3, 3.5b and 3.6b). To better understand whether there is a cause-effect relationship, we performed a time-course experiment on MCF-7 cells treated with DIM because unlike with I3C, DIM caused a reduction in both proliferation and FAS expression. The 48-h time course, however, indicates that a reduction in FAS expression may not necessarily be the cause of the inhibition of proliferation (Figure 3.4 a and b). Thus, at 12 h, MCF-7 cells have a significant reduction in growth compared to untreated cells. However, a reduction in FAS expression was significant only after 24 h of treatment with DIM. Hence, it appears that although
DIM causes a reduction in proliferation and FAS expression, the reduction in FAS expression may be a secondary effect that follows the reduction in proliferation.
We gained further evidence to support this notion from our rescue experiments.
Inhibition of FAS by I3C or DIM would reduce the over-production of palmitate by the cells.
Indeed, inhibition of FAS by cerulenin has been shown to reduce the amount of palmitate in
73
MCF-7 cells, resulting in supra-physiological accumulations of malonyl-CoA [105, 109].
However, studies showing a rescue effect of FAS-inhibited MCF-7 cells by palmitate have not been performed. Previously, it was shown in our lab that proliferation of MCF-7 cells treated with cerulenin can not be restored with 10-40 µM palmitate (unpublished data), and that greater than 40µM palmitate in the presence of cerulenin is toxic to the cells. Consistent with this finding, Figures 3.7 a and b show that supplementation of DIM-treated MCF-7 cells with 20 or
30 µM palmitate does not restore MCF-7 growth. (For the rescue experiments, we only attempted to restore proliferation of cells treated with DIM, not I3C, because of the greater suppression of MCF-7 proliferation observed with DIM). Since the addition of palmitate to the culture medium does not restore proliferation, this indicates that inhibition of proliferation may involve pathways other than FAS.
We also showed that DIM-treated MCF-7 cell proliferation is not restored when these cells are supplemented with oleate (Figure 3.7c). Menendez et al [165] have shown that oleate, a fatty acid generated de novo from palmitate, can rescue cerulenin-inhibited MCF-7, MDA-MB-
231 and SKBr-3 cell growth. However, several issues arise upon inspection of their analysis, mainly regarding the form and concentration of oleate used to restore cell proliferation. First,
Menendez et al treated the cells with a methyl ester of oleate, a form that would not likely be physiologically relevant. Second, they treated cells with a supraphysiologic concentration of oleate (500ug/ml), and we observed that this concentration was toxic to MCF-7 cells (data not shown). Third, oleate and palmitate are physiologically associated with the serum protein albumin, and Menendez et al did not include albumin in their culture medium. Hence, neither our results nor those in the literature support the notion that oleate restores MCF-7 cell proliferation after inhibition of FAS. Thus, although we showed that inhibition of cell growth by DIM is
74
associated with a reduction of FAS, DIM is likely acting upon other pathways to suppress cell
growth.
As mentioned in Chapter 1, the regulation and function of FAS differs between cancer
and non-cancer tissues. Most normal cells acquire fatty acids from the circulation and indeed,
MCF-10A cells express low levels of FAS. We showed that DIM had no effect on the
proliferation of these cells or on FAS expression (Figure 3.8). This further suggests that DIM
acts differentially on normal cells and cancer cells, since we showed a DIM-associated reduction
of FAS expression in all three cancer cell lines. As FAS over-expression is important to cancer
proliferation, but not to normal breast cell growth, we suggest that DIM may acting in cancer
cells to target FAS itself or genes involved in regulating FAS over-expression. However, in
Figure 3.9 we show that growth of MCF-7 cells is inhibited in the presence of the specific FAS inhibitor cerulenin, whereas growth of MCF-10A cells is unaffected by this compound. Because the inhibition of FAS activity differs between cancer and non-cancer cells, and since we showed that DIM reduces proliferation before significantly reducing FAS expression, we propose that inhibition of FAS expression may be a secondary effect of I3C and DIM treatment. In turn, we suggest that I3C and DIM may be acting on factor(s) upstream of FAS expression. Since we have previously shown FAS expression is regulated by the transcription factor Sp1, we next tested the effects I3C and DIM have on its expression.
As mentioned in Chapter 1, Sp1 has been shown to be over-expressed in several cancer cell lines [185-188]. Sp1 is necessary for the expression of several genes involved in cancer growth. For example, Sp1 sites have been found in the promoter regions of the CDK2, CDC25A,
CDK6 and p27 genes, all of which are necessary for G1 to S phase cell cycle progression [89,
92, 184]. As well, Sp1 sites have been found in genes important in cell survival such as Bcl-2,
Bcl-w and survivin [77]. Sp1 sites have also been located in the promoter region of the VEGF
75
and MMP-2 genes, which are necessary for angiogenesis and metastasis, respectively [189, 190,
195, 196] . Our lab has shown that binding of Sp1 to the promoter region of FAS is necessary for
its expression and for proliferation [184]. Hence, modification of the expression of Sp1 could
affect several genes important to cancer cell survival.
Our time-course experiment with MCF-7 cells indicates that at 24 h following DIM
treatment Sp1 levels are reduced by 84% (Figure 3.4c). We speculate that this large reduction in
Sp1 level may be responsible for the reduction in cell growth that we observed. Hence, we
propose that down-regulation of Sp1 by DIM causes a reduction of proliferation by modifying expression of several genes, including FAS. Real-time PCR, however, revealed that the DIM-
associated reduction of Sp1 protein level in MCF-7 cells is not due to a change at the transcript
level. Hence, DIM probably reduces Sp1 protein levels post-transcriptionally.
Furthermore, we showed that DIM caused a reduction in Sp1 expression in all three
cancer cell lines (Figures 3.3, 3.5c and 3.6c). Our early experiments tested the effect of I3C on
MCF-7 cells, but we did not observe a change FAS between treated and untreated cells. Hence,
we did not analyze Sp1 expression in MCF-7 cells after treatement with I3C. We have, on the
other hand, shown that I3C reduces Sp1 levels in MDA-MB-231 cells, but not in SKBr-3 cells
(Figures 3.5c and 3.6 c). Based on our results, it appears that I3C and DIM may be acting differentially on Sp1, since DIM, but not I3C, reduced Sp1 in all cancer cells. Thus, it seems likely that DIM, and not I3C, modifies Sp1-associated gene expression. Indeed DIM is known to accumulate in the nuclei of cells [77] and it has been suggested that I3C is converted to DIM before it enters into the nuclei of cells. Therefore, the effects that DIM may have on transcription factors could appear sooner than they would upon treatment with I3C. In summary, based on our data, DIM reduces Sp1 expression in breast cancer cells, but it is unclear whether I3C acts
76
similarly. Finally, our results indicate that DIM does not affect Sp1 expression in MCF-10A cells and also does not affect their proliferation (Figure 3.8).
Since we showed that Sp1 in normal cells is unaffected by DIM, but that DIM causes a downregulation of Sp1 protein in breast cancer cells, we suggest that the anticancer effect of
DIM may be due its action on down-regulating Sp1 protein. Hence, genes that are typically over- expressed in cancer and regulated by Sp1, such as FAS, CDC25A, CDK2 and 6, Bcl-2, and
VEGF are likely to be down-regulated upon treatment with DIM as a secondary effect of a reduction of Sp1 protein. In turn, several cellular processes imporortant to cancer cell growth, such as proliferation, apoptosis and angiogenesis would be affected (Figure 4.1).
Figure 4.1 - I3C/DIM modulates nuclear transcription factor Sp1, which is important in the regulation of several cancer genes and processes.
77
Conclusions
Our investigation was initially directed at understanding whether the anti-proliferative effect I3C and its condensation product DIM on cancer cells involves a change in the expression of FAS. Our results, however, have shown that the inhibitory effect of these indole compounds is more complex than we originally anticipated. Although DIM, and in some cases I3C, was associated with a reduction of FAS expression in breast cancer cells, the reduction in proliferation was likely not caused by changes in FAS, since reductions in FAS occur after a decrease in proliferation. DIM, and in some cases I3C, resulted in a down-regulation of Sp1, a transcription factor required for FAS expression. It seems likely that a reduction in Sp1 level would have caused a downregulation of several genes involved in cell cycle progression as well as in FAS. Interestingly, the effect that I3C and DIM have on cell growth appears to be specific for cancer cells, since these compounds did not appear to affect the growth, FAS or Sp1 levels of non-tumorigenic mammary epithelial cells.
Overall, our results suggest that I3C and DIM regulate Sp1 over-expression post- transcriptionally. Hence, the anticancer effect of these compounds may be due to their affect on several genes regulated by Sp1. Sp1-dependent genes such as FAS, CDK2 and 6, Bcl-2, and
VEGF have all been shown to be down-regulated upon treatment with I3C and DIM [77].
4.3 - Implications
Our findings may have implications for breast cancer therapy and prevention. Although
mortality from breast cancer has declined in the past decade due to advances in diagnosis and
treatment [210], clinical challenges still exist because of the development of drug resistance and
serious side effects [211]. Better approaches need to be developed. Sp1 is over-expressed in 80%
78
of breast carcinomas, and its expression is associated with poor prognosis [212]. As addressed in
Chapter 1, in breast cancer cells, Sp1 has been shown to play an important role in proliferation
[90, 184, 213], angiogenesis [189, 190], apoptosis [195], invasion and metastasis [196, 214]. Our
research has shown that dietary indole compounds significantly decrease the amount of Sp1
protein. Since Sp1 is crucial for maintaining multiple biological processes that are essential for
the survival and growth of cancer cells, our results suggest that this transcription factor is a
particularly promising target for breast cancer therapy.
4.4 – Limitations and Future Directions
Though our results are consistent with previous findings for the anti-proliferative effect
of I3C/DIM on cultured breast cancer cells, and though our results provide insight into the
mechanistic relationship of this effect, several limitations to our study should be considred. First,
although we have linked our proliferation assays to our western blots, the diameter of the culture
dishes used, and hence the number of cells tested for each assay, differed. We used
materials/techniques that were readily available in our lab, however, dish diameters of equal
lengths would allow us to assess the associations we observed with greater certainty. Secondly,
though literature values have tested these compounds with cell passage generations of less than
20, we specifically used between 4-7, for the most part, and up to 12 for our cerulenin experiments on MCF-10A cells. Although we are unaware of the effect on cell physiology between 4-12 and 20 passages for each of the four cell lines, our results could possibly have been more comparable to literature values had these parameters been the same.
Furthermore, several possible limitations could be considered for our time-course experiment. First, it would have been interesting to know how DIM affects proliferation and Sp1
79
in MDA-MB-231 and SKBr-3 cells over the 48-h period, along with our MCF-7 cell results. We
could better understand the relationship between DIM, proliferation and Sp1 by looking for
similar trends (to our MCF-7 results) across a larger number of breast cancer cell types. As well,
there may also have been issues with the number of time points we had for our time-course experiment and/or the duration of each interval. Had we measured more intervals over the first
24 h, we could better understand the relationship between the reduction in proliferation and the reduction in Sp1 soon after treatment. As well, we could also be more confident in our time-
course results had we repeated this experiment at least one more time. Variability in the pipetting
of MCF-7 protein, as well as in the densitometry technique we used likely exist, hence,
replication of our results could give us greater confidence in our observations.
Finally, another possible limitation to our study could be that we tested the effect DIM
has on one non-cancer cell line, MCF-10A. In line with out results, it has been previously shown
that DIM does not affect growth of this cell line, but the absorbtion of DIM into this cell line is
not known. It is possible that this cell line may be more resistant to the absorption of DIM.
Performing a similar experiment across more non-cancer mammary cell lines could provide more
evidence to our hypothesis, that DIM acts specifically to reduce the proliferation of breast cancer
cells by a reduction in Sp1, and does not do the same to non-cancer mammary cells.
Our study has provided a strong case in favor of further exploring the effect that I3C and
DIM have on Sp1 and its associated proteins in cancer. While we have been able to show that
DIM and in some cases I3C reduce the total amount of Sp1 protein in treated cancer cells, we
showed that this effect is not at the Sp1 transcript level. We speculate that I3C and DIM could be
activating mechanisms that lead to the degradation of Sp1 protein. This degradation mechanism
should be further investigated. Since Sp1 is known to undergo ubiquitination [215] (which refers
to its post-translational proteosomal degradation by the attachment of one or more ubiquitin
80 monomers), one possible experiment could involve the inhibition of this process with the cell- permeable proteasome inhibitor MG132. It would be particularly interesting to see if inhibition of Sp1 degradation would reduce I3C and DIM’s anti-proliferative effect. Furthermore, it would be interesting to know how genes that are down-regulated by treatment of these indoles (e.g.
FAS), would be affected by inhibition of Sp1 degradation.
As well as reducing MCF-7 and MDA-MB-231 proliferation, both these compounds have been shown to increase the level of apoptosis in these cell lines [77]. Since Bcl-2, a major enzyme controlling apoptosis, also requires Sp1, it would be interesting to test whether its downregulation of Bcl-2 was also caused by these indoles. For this, a time-course experiment similar to the one we prepared for DIM on MCF-7 cells could be performed. Results from this experiment could provide more substance to our notion that a reduction in Sp1 affects several important genes in cancer cells.
Furthermore our study focused on breast cancer cells, but future in vitro experiments should also include cell lines that are derived from other cancers such as prostate, colon, endometrial and lung cancer.
REFERENCES
81
82
1. NCIC, Canadian Cancer Statistics. National Cancer Institute of Canada, 2009. 2. Parkin, D., et al. Global Cancer Statistics, 2002. Cancer J Clin, 2005. 55: p. 74-108. 3. McMichael, A., et al. Cancer in migrants to Australia: extending the descriptive epidemiological data. Cancer Res, 1988. 48(3): p. 751-6. 4. Ziegler, R., et al. Migration patterns and breast cancer risk in Asian-American women. J Natl Cancer Inst, 1993. 85(22): p. 1819-27. 5. Shimizu, H. et al. Cancers of the prostate and breast among Japanese and white immigrants in Los Angeles County. Br J Cancer, 1991. 63(6): p. 963-6. 6. Kolonel, L.N. Cancer patterns of four ethnic groups in Hawaii. J Natl Cancer Inst, 1980. 65(5): p. 1127-39. 7. AICR, W. Food, Nutrition and the Prevention of Cancer: a global perspective. Washing, D.C., American Institute for Cancer Research., 1997. 8. Armstrong, B., et al. Environmental factors and cancer incidence and mortality in different countries, with special reference to dietary practices. Int J Cancer, 1975. 15(4): p. 617-31. 9. Sim, H.G. and C.W. Cheng. Changing demography of prostate cancer in Asia. Eur J Cancer, 2005. 41(6): p. 834-45. 10. Deapen, D., et al. Rapidly rising breast cancer incidence rates among Asian-American women. Int J Cancer, 2002. 99(5): p. 747-50. 11. WHO, The World Health Report Geneva: WHO. 1997. 12. Gopalan, G. Diet Nutrition and Chronic Disease - Lessons from Contrasting Worlds. PShetty, PS; McPherson, K (eds), 1997.
13. Willett, W.C. Diet and cancer. Oncologist, 2000. 5(5): p. 393-404. 14. Beliveau, R. and D. Gingras. Role of nutrition in preventing cancer. Can Fam Physician, 2007. 53(11): p. 1905-11. 15. Michels, K., et al. Diet and breast cancer: a review of the prospective observational studies. Cancer, 2007. 109(12 Suppl): p. 2712-49. 16. Smith-Warner, S.A., et al. Alcohol and breast cancer in women: a pooled analysis of cohort studies. Jama, 1998. 279(7): p. 535-40. 17. Wu, A.H., et al. Meta-analysis: dietary fat intake, serum estrogen levels, and the risk of breast cancer. J Natl Cancer Inst, 1999. 91(6): p. 529-34. 18. Zhang, S., et al. Dietary carotenoids and vitamins A, C, and E and risk of breast cancer. J Natl Cancer Inst, 1999. 91(6): p. 547-56. 19. Holmes, M.D., et al. Dietary carbohydrates, fiber, and breast cancer risk. Am J Epidemiol, 2004. 159(8): p. 732-9.
83
20. Wu, A.H., et al. Epidemiology of soy exposures and breast cancer risk. Br J Cancer, 2008. 98(1): p. 9-14. 21. Wang, Y., et al. The red wine polyphenol resveratrol displays bilevel inhibition on aromatase in breast cancer cells. Toxicol Sci, 2006. 92(1): p. 71-7. 22. Etminan, M., et al. The role of tomato products and lycopene in the prevention of prostate cancer: a meta-analysis of observational studies. Cancer Epidemiol Biomarkers Prev, 2004. 13(3): p. 340-5. 23. Etminan, M., et al. Intake of selenium in the prevention of prostate cancer: a systematic review and meta-analysis. Cancer Causes Control, 2005. 16(9): p. 1125-31. 24. Cohen J.H., et al.Fruit and vegetable intakes and prostate cancer risk. J Natl Cancer Inst, 2000. 92(1): p.61-8. 25. Michaud D.S., et al. Fruit and vegetable intake and incidence of bladder cancer in a male prospective cohort. J Natl Cancer Inst, 1999. 91(7): p.605-13. 26. Verhoeven D.T., et al. Epidemiological studies on brassica vegetables and cancer risk. Cancer Epidemiol Biomarkers Prev, 1996. 9 p.733-48. 27. Higdon, J.V., et al.Cruciferous vegetables and human cancer risk: epidemiologic evidence and mechanistic basis. Pharmacol Res, 2007. 55 (3): p224-36. 28. Keck A.S., and Finley, J.W. Cruciferous vegetables: cancer protective mechanisms of glucosinolate hydrolysis products and selenium. Integr Cancer Ther, 2004. 1 p. 5-12. 29. Hayes J.D., Kelleher, M.O., and Eggleston I.M. The cancer chemopreventive actions of phytochemicals derived from glucosinolates. Eur J Nutr, 2008. 47 Suppl 2: p.73-88. 30. Johnson, I.T. Glucosinolates: bioavailability and importance to health. Int J Vitam Nutr Res, 2002. 72(1): p. 26-31. 31. Verkerk R., et al. Glucosinolates in Brassica vegetables: The influence of the food supply chain on intake, bioavailability and human health. Mol Nutr Food Res, 2008. 32. Carlson, D., et al. Glucosinolates in crucifer vegetables: broccoli, Brussels sprouts, cauliflower, collard, kale, mustard greens, and kohlrabi. J Am Soc Hortic Sci. 1987b. 112: p 173-178. 33. Padilla G., et al. Variation of glucosinolates in vegetable crops of Brassica rapa. Phytochemistry, 2007. 68(4): p. 536-45. 34. Kushad, M.M., et al. Variation of glucosinolates in vegetable crops of Brassica oleracea. J Agric Food Chem, 1999. 47(4): p. 1541-8. 35. Shelp, B., et al. Glucosinolate composition of broccoli grown under various boron treatments at three Ontario sites. Can J Plant Sci, 1993. 73: p. 885-888. 36. Fenwick, G.R., Heaney, R.K., and Mullin, W.J. Glucosinolates and their breakdown products in food and food plants. Crit Rev Food Sci Nutr, 1983. 18(2): p. 123-201.
84
37. Ludikhuyze, L., Rodrigo, L., and Hendrickx, M. The activity of myrosinase from broccoli (Brassica oleracea L. cv. Italica): influence of intrinsic and extrinsic factors. J Food Prot, 2000. 63(3): p. 400-3. 38. Rungapamestry, V. et al. Effect of cooking brassica vegetables on the subsequent hydrolysis and metabolic fate of glucosinolates. Proc Nutr Soc, 2007. 66(1): p. 69-81. 39. Yen, G., and Wei, Q. Myrosinase activity and total glucosinolate content of cruciferous vegetables, and some properties of cabbage myrosinase in Taiwon. J Sci Food & Agric, 1993. 61: p. 471-475. 40. Ludikhuyze, L., et al. Kinetic study of the irreversible thermal and pressure inactivation of myrosinase from broccoli. J Food Prot, 1999. 63: p. 400-403. 41. Rouzaud, G., et al. Influence of plant and bacterial myrosinase activity on the metabolic fate of glucosinolates in gnotobiotic rats. Br J Nutr, 2003. 90(2): p. 395-404. 42. Krul, C., et al. Metabolism of sinigrin (2-propenyl glucosinolate) by the human colonic microflora in a dynamic in vitro large-intestinal model. Carcinogenesis, 2002. 23(6): p. 1009-16. 43. Telang, U., Brazeau, D.A., and Morris, M.E. Comparison of the effects of phenethyl isothiocyanate and sulforaphane on gene expression in breast cancer and normal mammary epithelial cells. Exp Biol Med (Maywood), 2009. 234(3): p. 287-95. 44. Lee, J.W., and Cho, M.K. Phenethyl isothiocyanate induced apoptosis via down regulation of Bcl-2/XIAP and triggering of the mitochondrial pathway in MCF-7 cells. Arch Pharm Res, 2008. 31(12): p. 1604-12. 45. Stoner, G.D., et al. Carcinogen-altered genes in rat esophagus positively modulated to normal levels of expression by both black raspberries and phenylethyl isothiocyanate. Cancer Res, 2008. 68(15): p. 6460-7. 46. Cuddihy, S.L., et al. Induction of apoptosis by phenethyl isothiocyanate in cells overexpressing Bcl-XL. Cancer Lett, 2008. 271(2): p. 215-21. 47. Jackson, S.J., and Singletary, K.W. Sulforaphane inhibits human MCF-7 mammary cancer cell mitotic progression and tubulin polymerization. J Nutr, 2004. 134(9): p. 2229-36. 48. Fimognari, C. et al. Growth inhibition, cell-cycle arrest and apoptosis in human T-cell leukemia by the isothiocyanate sulforaphane. Carcinogenesis. 2002. 23(4): p. 581-6. 49. Wang, L., et al. Targeting cell cycle machinery as a molecular mechanism of sulforaphane in prostate cancer prevention. Int J Oncol, 2004. 24(1): p. 187-92. 50. Minich, D.M., and Bland, J.S. A review of the clinical efficacy and safety of cruciferous vegetable phytochemicals. Nutr Rev, 2007. 65(6 Pt 1): p. 259-67. 51. Anderton, M., et al. Pharmacokinetics and tissue disposition of indole-3-carbinol and its acid condensation products after oral administration to mice. Clinical Cancer Research, 2004. 10: p. 5233–5241.
85
52. Howells, L.M., et al. Inhibition of phosphati-dylinositol 3-kinase/protein kinase B signaling is not sufficient to account for indole-3-carbinol-induced apoptosis in some breast and prostate tumor cells. Clin Cancer Res, 2005. 11: p. 8521–27. 53. Broadbent, T,A, and Broadbent, H.S. The chemistry and pharmacology of indole-3- carbinol (indole-3-methanol) and 3-(methoxymethyl)indole. Cur Med Chem 1988. 5: p. 337–352.
54. Sones, K., Heaney, R., and Fenwick, G. An estimate of the mean daily intake of glucosinolates from cruciferous vegetables in the UK. J Sci, Food & Agri, 1984. 35: p. 712–720.
55. Hecht, S., et al. Effects of cruciferous vegetable consumption on urinary metabolites of the tobacco-specific lung carcinogen 4-(methylnitrosamino)-1-(3-pyridyl)-1-butanone in Singapore Chinese. Cancer Epid, Biom & Prev, 2004. 13: p. 997–1004.
56. Grubbs, C.J., et al. Chemoprevention of chemically-induced mammary carcinogenesis by indole-3-carbinol. Anticancer Res, 1995. 15(3): p. 709-16.
57. Bradlow, H.L., et al. Effects of dietary indole-3-carbinol on estradiol metabolism and spontaneous mammary tumors in mice. Carcinogenesis, 1991. 9: p. 1571-4.
58. Manson, M.M., et al. Chemoprevention of aflatoxin B1-induced carcinogenesis by indole-3-carbinol in rat liver--predicting the outcome using early biomarkers. Carcinogenesis, 1998. 19(10): p. 1829-36.
59. Morse, M.A., et al. Effects of indole-3-carbinol on lung tumorigenesis and DNA methylation induced by 4-(methylnitrosamino)-1-(3-pyridyl)-1-butanone (NNK) and on the metabolism and disposition of NNK in A/J mice. Cancer Res, 1990. 50(9): p. 2613-7.
60. Kassie, F.,et al. Dose-dependent inhibition of tobacco smoke carcinogen-induced lung tumorigenesis in A/J mice by indole-3-carbinol. Cancer Prev Res, 2007. 7: p. 568-76.
61. Tanaka, T., Kojima, T., Morishita, Y., and Mori, H. Inhibitory effects of the natural products indole-3-carbinol and sinigrin during initiation and promotion phases of 4- nitroquinoline 1-oxide-induced rat tongue carcinogenesis. Jpn J Cancer Res, 1992. 83(8): p. 835-42.
62. Kojima, T., Tanaka, T., and Mori, H. Chemoprevention of spontaneous endometrial cancer in female Donryu rats by dietary indole-3-carbinol. Cancer Res, 1994. 54(6): p. 1446-9.
63. Jin, L., et al. Indole-3-carbinol prevents cervical cancer in human papilloma virus type 16 (HPV16) transgenic mice. Cancer Res. 1999. 59(16): p. 3991-7.
64. Chen, I., McDougal, A., Wang, F., and Safe, S. Aryl hydrocarbon receptor-mediated antiestrogenic and antitumorigenic activity of diindolylmethane. Carcinogenesis, 1998. 19(9): p. 1631-9.
86
65. Chang, X., Firestone, G.L., Bjeldanes, L.F, et al. 3,3'-Diindolylmethane inhibits angiogenesis and the growth of transplantable human breast carcinoma in athymic mice. Carcinogenesis, 2005. 4: p. 771-8.
66. Chang Y.C., Riby J., Chang, G.H., Peng, B,C,, Firestone, G., and Bjeldanes, L.F. Cytostatic and antiestrogenic effects of 2-(indol-3-ylmethyl)-3,3'-diindolylmethane, a major in vivo product of dietary indole-3-carbinol. Biochem Pharmacol, 1999. 58(5): p. 825-34.
67. McDougal, A., et al. Methyl-substituted diindolylmethanes as inhibitors of estrogen- induced growth of T47D cells and mammary tumors in rats. Breast Cancer Res Treat, 2001. 66(2):147-57.
68. Kim, Y.H., et al. 3,3'-diindolylmethane attenuates colonic inflammation and tumorigenesis in mice. Inflamm Bowel Dis, 2009. 15(8): p. 1164-73.
69. Kassie, F., et al. Indole-3-carbinol inhibits 4-(methylnitrosamino)-1-(3-pyridyl)-1- butanone plus benzo(a)pyrene-induced lung tumorigenesis in A/J mice and modulates carcinogen-induced alterations in protein levels. Cancer Res, 2008. 67(13): p. 6502-11.
70. Nachshon-Kedmi, M., Fares, F.A, and Yannai, S. Therapeutic activity of 3,3'- diindolylmethane on prostate cancer in an in vivo model. Prostate, 2004. 61(2): p.153-60.
71. Reed, G.A., et al. A phase I study of indole-3-carbinol in women: tolerability and effects. Cancer Epidemiol Biomarkers Prev, 2005. 14(8): p. 1953-60.
72. Reed, G.A., et al. Single-dose and multiple-dose administration of indole-3-carbinol to women: pharmacokinetics based on 3,3'-diindolylmethane. Cancer Epidemiol Biomarkers Prev, 2006. 15(12): p. 2477-81.
73. Qi, M., et al. Indole-3-carbinol prevents PTEN loss in cervical cancer in vivo. Mol Med, 2005. 11(1-12): p. 59-63.
74. Naik, R., et al. A randomized phase II trial of indole-3-carbinol in the treatment of vulvar intraepithelial neoplasia. Int J Gynecol Cancer, 2006. 16(2): p. 786-90.
75. Bell, M.C., et al. Placebo-controlled trial of indole-3-carbinol in the treatment of CIN. Gynecol Oncol, 2000. 78(2): p. 123-9.
76. Kietpeerakool, C., and Srisomboon, J. Medical treatment of cervical intraepithelial neoplasia II, III: an update review. Int J Clin Oncol, 2009. 14(1): p. 37-42.
77. Kim. Y.S., and Milner, J.A. Targets for indole-3-carbinol in cancer prevention. J Nutr Biochem, 2005. 16(2): p. 65-73.
78. Meng, Q., et al. Indole-3-Carbinol is a negative regulator of estrogen receptor-alpha signaling in human tumor cells. J Nutr, 2000. 130: p. 2927-2931.
87
79. Le, H., Firestone, G., Bjeldanes., L.F., et al Plant-derived 3,3’-diindolylmethane is a strong androgen antagonist in human prostate cells. J Biol Chem, 2003. 278: p. 21136- 21145.
80. Hsu, J., Bjeldanes, L., Firestone, et al. G. Indole-3-carbinol inhibition of androgen receptor expression and down-regulation of androgen resposiveness in human prostate cancer cells. Carcinogenesis, 2005. 26: p. 1896-1904.
81. Sundar, S.N, Bjeldanes, L.F., Firestone, G.L., et al Indole-3-carbinol selectively uncouples expression and activity of estrogen receptor subtypes in human breast cancer cells. Mol Endocr, 2006. 20: p. 3070–82.
82. Moiseeva, E.P., et al. Indole-3-carbinol-induced death in cancer cells involves EGFR downregulation and is exacerbated in a 3D environment. Apoptosis, 2006. 11: p. 799– 812.
83. Fan, S., et al. BRCA1 and BRCA2 as molecular targets for phytochemicals indole-3- carbinol and genistein in breast and prostate cancer cells. Brit J Cancer, 2006. 94: p. 407–26.
84. Ociepa-Zawal, M., et al. The effect of indole-3-carbinol on the expression of CYP1A1, CYP1B1, and AhR genes and proliferation of MCF-7 cells. Acta Bioch Pol. 2007. 54: p. 113-117.
85. Horn, T., et al. Modulations of P450 mRNA in liver and mammary gland and P450 activities and metabolism of estrogen in liver by treatment of rats with indole-3- carbinole. Biochem Pharm, 2002. 64: p. 393-404.
86. Rahman, K., Li, Y., and Sarkar, F. Inactivation of Akt and NF-kappaB play important roles during indole-3-carbinol induced apoptosis in breast cancer cells. Nutr Cancer, 2004. 48: p. 84-94.
87. Sarkar, F., Rahman, K., and Li, Y. Bax translocation to mitochondria is an important event in inducing apoptotic cell death by indole-3-carbinol treatment of breast cancer cells. J Nutr, 2003. 133: p. 2434s-2439s.
88. Safe, S., and Abdelrahim, M. Sp transcription factor family and its role in cancer. European J Cancer, 2005. 41: p. 2438-2448.
89. Cram, E., Liu, B., Bjeldanes, L., and Firestone, G. Indole-3-Carbinol inhibits CDK6 expression in human MCF-7 breast cancer cells by disrupting Sp1 transcription factor interactions with a composite element in the CDK6 gene promoter. J Biol Chem, 2001. 276: p. 22332-22340.
90. Hong, C., Kim, H., Firestone, G., and Bjeldanes, L. 3,3’-Diindolyl methane induces G1 cell cycle arrest in human breast cancer cells that is accompanied by Sp1-mediated activation of p21 WAF/CIP1 expression. Carcinogenesis, 2001. 23: p. 1297-305.
88
91. Cover, C.M., Bjeldanes L.F., Firestone G.L., et al. Indole-3-carbinol inhibits the expression of cyclin-dependent kinase-6 and induces a G1 cell cycle arrest of human breast cancer cells independent of estrogen receptor signaling. J Biol Chem. 1998. 13;273(7): p. 3838-47.
92. Firestone, G.L., and Bjeldanes, L.F. Indole-3-carbinol and 3-3'-diindolylmethane antiproliferative signaling pathways control cell-cycle gene transcription in human breast cancer cells by regulating promoter-Sp1 transcription factor interactions. J Nutr. 2003. 133: p. 2448S-2455S.
93. Brew, C.T., Bjeldanes, L.F., Firestone, G.L, et al. Indole-3-carbinol inhibits MDA-MB- 231 breast cancer cell motility and induces stress fibers and focal adhesion formation by activation of Rho kinase activity. Int J Cancer. 2009. 15;124(10): p. 2294-302.
94. Nguyen, H.H., Bjeldanes, L.F., Firestone, G.L., et al. The dietary phytochemical indole- 3-carbinol is a natural elastase enzymatic inhibitor that disrupts cyclin E protein processing. Proc Natl Acad Sci, 2008. 105(50): p. 19750-5.
95. Sul, H. et al Nutritional and hormonal regulation of enzymes in fat synthesis: studies of fatty acid synthesis and mitochondrial glycerol-3-phosphate acyltransferase gene transcription. Annu. Rev. Nutr., 1998. 18: p. 331-351. 96. Chirala, S.S., et al., Human fatty acid synthase: role of interdomain in the formation of catalytically active synthase dimer. Proc Natl Acad Sci U S A, 2001. 98(6): p. 3104-8. 97. Smith, S., The animal fatty acid synthase: one gene, one polypeptide, seven enzymes. Faseb J, 1994. 8(15): p. 1248-59. 98. Wakil, S.J., Fatty acid synthase, a proficient multifunctional enzyme. Biochemistry, 1989. 28(11): p. 4523-30. 99. Weiss, L., et al., Fatty-acid biosynthesis in man, a pathway of minor importance. Purification, optimal assay conditions, and organ distribution of fatty-acid synthase. Biol Chem Hoppe Seyler, 1986. 367(9): p. 905-12. 100. Menendez, J.A., R. Colomer, and R. Lupu, Why does tumor-associated fatty acid synthase (oncogenic antigen-519) ignore dietary fatty acids? Med Hypotheses, 2005. 64(2): p. 342-9. 101. Hillgartner, F., et al. Physiological and molecular mechanisms involved in nutritional regulation of fatty acid synthesis. Physiol Rev, 1995. 75: 47-76. 102. Chakravarthy, M.V., et al., "New" hepatic fat activates PPARalpha to maintain glucose, lipid, and cholesterol homeostasis. Cell Metab, 2005. 1(5): p. 309-22.
103. Kim, K.H., Regulation of mammalian acetyl-coenzyme A carboxylase. Annu Rev Nutr, 1997. 17: p. 77-99.
104. Omura, S., The antibiotic cerulenin, a novel tool for biochemistry as an inhibitor of fatty acid synthesis. Bacteriol Rev, 1976. 40(3): p. 681-97.
89
105. Funabashi, H., et al., Binding site of cerulenin in fatty acid synthetase. J Biochem (Tokyo), 1989. 105(5): p. 751-5.
106. Pizer, E.S., et al., Inhibition of fatty acid synthesis delays disease progression in a xenograft model of ovarian cancer. Cancer Res, 1996. 56(6): p. 1189-93.
107. Furuya, Y., et al., Apoptosis of androgen-independent prostate cell line induced by inhibition of fatty acid synthesis. Anticancer Res, 1997. 17(6D): p. 4589-93.
108. Pizer, E.S., et al., Pharmacological inhibitors of mammalian fatty acid synthase suppress DNA replication and induce apoptosis in tumor cell lines. Cancer Res, 1998. 58(20): p. 4611-5.
109. Dridi, S., et al., FAS inhibitor cerulenin reduces food intake and melanocortin receptor gene expression without modulating the other (an)orexigenic neuropeptides in chickens. Am J Physiol Regul Integr Comp Physiol, 2006. 291(1): p. R138-47.
110. Loftus, T.M., et al., Reduced food intake and body weight in mice treated with fatty acid synthase inhibitors. Science, 2000. 288(5475): p. 2379-81.
111. Kuhajda, F.P., Fatty-acid synthase and human cancer: new perspectives on its role in tumor biology. Nutrition, 2000. 16(3): p. 202-8.
112. Rendina, A.R. and D. Cheng, Characterization of the inactivation of rat fatty acid synthase by C75: inhibition of partial reactions and protection by substrates. Biochem J, 2005. 388(Pt 3): p. 895-903.
113. Kuhajda, F.P., et al., Synthesis and antitumor activity of an inhibitor of fatty acid synthase. Proc Natl Acad Sci U S A, 2000. 97(7): p. 3450-4.
114. Guerciolini, R., Mode of action of orlistat. Int J Obes Relat Metab Disord, 1997. 21 Suppl 3: p. S12-23.
115. Kridel, S.J., et al., Orlistat is a novel inhibitor of fatty acid synthase with antitumor activity. Cancer Res, 2004. 64(6): p. 2070-5.
116. Menendez, J.A., L. Vellon, and R. Lupu, Orlistat: from antiobesity drug to anticancer agent in Her-2/neu (erbB-2)-overexpressing gastrointestinal tumors? Exp Biol Med (Maywood), 2005. 230(3): p. 151-4.
117. Hursting, S.D., M. Thornquist, and M.M. Henderson, Types of dietary fat and the incidence of cancer at five sites. Prev Med, 1990. 19(3): p. 242-53.
118. Bhargava, H.N. and P.A. Leonard, Triclosan: applications and safety. Am J Infect Control, 1996. 24(3): p. 209-18.
119. Rock, C.O. and J.E. Cronan, Escherichia coli as a model for the regulation of dissociable (type II) fatty acid biosynthesis. Biochim Biophys Acta, 1996. 1302(1): p. 1- 16.
120. Liu, B., et al., Triclosan inhibits enoyl-reductase of type I fatty acid synthase in vitro and is cytotoxic to MCF-7 and SKBr-3 breast cancer cells. Cancer Chemother Pharmacol, 2002. 49(3): p. 187-93.
90
121. Lu, S. and M.C. Archer, Fatty acid synthase is a potential molecular target for the chemoprevention of breast cancer. Carcinogenesis, 2005. 26(1): p. 153-7.
122. Brusselmans, K., et al., Induction of cancer cell apoptosis by flavonoids is associated with their ability to inhibit fatty acid synthase activity. J Biol Chem, 2005. 280(7): p. 5636-45.
123. Tian, W.X., Inhibition of fatty acid synthase by polyphenols. Curr Med Chem, 2006. 13(8): p. 967-77.
124. Liu, L. and Y.Y. Yeh, Water-soluble organosulfur compounds of garlic inhibit fatty acid and triglyceride syntheses in cultured rat hepatocytes. Lipids, 2001. 36(4): p. 395- 400.
125. Yasni, S., et al., Effects of Curcuma xanthorrhiza Roxb. and curcuminoids on the level of serum and liver lipids, serum apolipoprotein A-I and lipogenic enzymes in rats. Food Chem Toxicol, 1993. 31(3): p. 213-8.
126. Ide, T., et al., Sesamin, a sesame lignan, decreases fatty acid synthesis in rat liver accompanying the down-regulation of sterol regulatory element binding protein-1. Biochim Biophys Acta, 2001. 1534(1): p. 1-13. 127. Tian, W.X., et al., Weight reduction by Chinese medicinal herbs may be related to inhibition of fatty acid synthase. Life Sci, 2004. 74(19): p. 2389-99.
128. Voet, D and Voet J. Fundamentals of Biochemistry: Regulation of Fatty Acid Metabolism. Copyright Wiley & Sons, Inc. Seattle, Washington. 2002. p. 585-595.
129. Lakshmanan, M.R., C.M. Nepokroeff, and J.W. Porter, Control of the synthesis of fatty- acid synthetase in rat liver by insulin, glucagon, and adenosine 3':5' cyclic monophosphate. Proc Natl Acad Sci U S A, 1972. 69(12): p. 3516-9.
130. Claycombe, K.J., et al., Insulin increases fatty acid synthase gene transcription in human adipocytes. Am J Physiol, 1998. 274(5 Pt 2): p. R1253-9.
131. Moustaid, N., B.H. Jones, and J.W. Taylor, Insulin increases lipogenic enzyme activity in human adipocytes in primary culture. J Nutr, 1996. 126(4): p. 865-70.
132. Anderson, S., et al. Key stages in mammary gland development. Secretory activation in the mammary gland: it’s not just about milk protein synthesis! Breast Cancer Res. 2007. 9: p. 204-205.
133. Pizer, E., et al. Expression of fatty acid synthase is closely linked to proliferation and stromal decidualization in cycling endometrium. Int. J. Gynecol. Pathol., 1997. 16 p. 45- 51.
134. Brown, M.S. and J.L. Goldstein, The SREBP pathway: regulation of cholesterol metabolism by proteolysis of a membrane-bound transcription factor. Cell, 1997. 89(3): p. 331-40.
91
135. Shimomura, I., et al., Differential expression of exons 1a and 1c in mRNAs for sterol regulatory element binding protein-1 in human and mouse organs and cultured cells. J Clin Invest, 1997. 99(5): p. 838-45.
136. Shimano, H., et al., Sterol regulatory element-binding protein-1 as a key transcription factor for nutritional induction of lipogenic enzyme genes. J Biol Chem, 1999. 274(50): p. 35832-9.
137. Liang, G., et al., Diminished hepatic response to fasting/refeeding and liver X receptor agonists in mice with selective deficiency of sterol regulatory element-binding protein- 1c. J Biol Chem, 2002. 277(11): p. 9520-8.
138. Shimano, H., et al., Isoform 1c of sterol regulatory element binding protein is less active than isoform 1a in livers of transgenic mice and in cultured cells. J Clin Invest, 1997. 99(5): p. 846-54.
139. Shimomura, I., et al., Nuclear sterol regulatory element-binding proteins activate genes responsible for the entire program of unsaturated fatty acid biosynthesis in transgenic mouse liver. J Biol Chem, 1998. 273(52): p. 35299-306.
140. Latasa, M.J., et al., Nutritional regulation of the fatty acid synthase promoter in vivo: sterol regulatory element binding protein functions through an upstream region containing a sterol regulatory element. Proc Natl Acad Sci U S A, 2000. 97(19): p. 10619-24.
141. Griffin, M.J. and H.S. Sul, Insulin regulation of fatty acid synthase gene transcription: roles of USF and SREBP-1c. IUBMB Life, 2004. 56(10): p. 595-600.
142. Sawadogo, M. and R.G. Roeder, Interaction of a gene-specific transcription factor with the adenovirus major late promoter upstream of the TATA box region. Cell, 1985. 43(1): p. 165-75.
143. Wang, D. and H.S. Sul, Upstream stimulatory factor binding to the E-box at -65 is required for insulin regulation of the fatty acid synthase promoter. J Biol Chem, 1997. 272(42): p. 26367-74.
144. Moon, Y.S., et al., Two 5'-regions are required for nutritional and insulin regulation of the fatty-acid synthase promoter in transgenic mice. J Biol Chem, 2000. 275(14): p. 10121-7.
145. Casado, M., et al., Essential role in vivo of upstream stimulatory factors for a normal dietary response of the fatty acid synthase gene in the liver. J Biol Chem, 1999. 274(4): p. 2009-13.
146. Oka, S., et al. NMR Structure of transcription factor Sp1 DNA binding domain. Biochemistry, 2004. 43: p. 16027-16035.
147. Wolf SS, Roder K, and Schweizer M. Role of Sp1 and Sp3 in the transcriptional regulation of the fatty acid synthase gene. Arch Biochem Biophys, 2001. 385(2): p. 259- 66.
92
148. Wierstra I. Sp1: emerging roles--beyond constitutive activation of TATA-less housekeeping genes. Biochem Biophys Res Commun. 2008. 18;372(1): p. 1-13.
149. Marin, M., et al. Transcription factor Sp1 is essential for early embryonic development but dispensible for cell growth and differentiation. Cell, 1997. 89: p. 619-628.
150. Bouman, P., et al. Transcription factor Sp1 is essential for post-natal survival and late tooth development. EMBO J, 2000. 19: p. 655-661.
151. Gollner, H., et al. Impaired ossification in mice lacking the transcription factor Sp1. Mech Dev, 2001. 106: p. 77-83.
152. Kuhajda, F., et al. Haptoglobin-related protein (Hpr) epitopes in breast cancer as a predictor of recurrence of the disease. N Eng J Med, 1989. 321: p. 636-641.
153. Epstein, J.I., M. Carmichael, and A.W. Partin, OA-519 (fatty acid synthase) as an independent predictor of pathologic state in adenocarcinoma of the prostate. Urology, 1995. 45(1): p. 81-6.
154. Shurbaji, M.S., J.H. Kalbfleisch, and T.S. Thurmond, Immunohistochemical detection of a fatty acid synthase (OA-519) as a predictor of progression of prostate cancer. Hum Pathol, 1996. 27(9): p. 917-21.
155. Milgraum, L.Z., et al., Enzymes of the fatty acid synthesis pathway are highly expressed in in situ breast carcinoma. Clin Cancer Res, 1997. 3(11): p. 2115-20.
156. Gansler, T.S., et al., Increased expression of fatty acid synthase (OA-519) in ovarian neoplasms predicts shorter survival. Hum Pathol, 1997. 28(6): p. 686-92.
157. Alo, P.L., et al., Fatty acid synthase (FAS) predictive strength in poorly differentiated early breast carcinomas. Tumori, 1999. 85(1): p. 35-40.
158. Pizer, E.S., et al., Fatty acid synthase expression in endometrial carcinoma: correlation with cell proliferation and hormone receptors. Cancer, 1998. 83(3): p. 528-37.
159. Rashid, A., et al., Elevated expression of fatty acid synthase and fatty acid synthetic activity in colorectal neoplasia. Am J Pathol, 1997. 150(1): p. 201-208.
160. Piyathilake, C.J., et al., The expression of fatty acid synthase (FASE) is an early event in the development and progression of squamous cell carcinoma of the lung. Hum Pathol, 2000. 31(9): p. 1068-73.
161. Kusakabe, T., et al., Fatty acid synthase is highly expressed in carcinoma, adenoma and in regenerative epithelium and intestinal metaplasia of the stomach. Histopathology, 2002. 40(1): p. 71-799.
162. Hennigar, R., et al. Characterization of fatty acid synthase in cell lines derived from experimental mammary tumors. Biochim Biophys Acta, 1998. 1392: p. 85-100.
163. Alli, P., et al. Fatty acid synthase inhibitors are chemopreventive for mammary cancer in neu-N transgenic mice. Oncogene, 2005. 24: p. 39-46.
93
164. Cognault, S., et al. Fatty acid synthase gene expression in rat mammary carcinoma. Lipids, 1999. 34 Suppl: p. S223.
165. Menendez, J.A., et al., Novel signaling molecules implicated in tumor-associated fatty acid synthase-dependent breast cancer cell proliferation and survival: Role of exogenous dietary fatty acids, p53-p21WAF1/CIP1, ERK1/2 MAPK, p27KIP1, BRCA1, and NF-kappaB. Int J Oncol, 2004. 24(3): p. 591-608.
166. Hochachka, P.W., et al., Going malignant: the hypoxia-cancer connection in the prostate. Bioessays, 2002. 24(8): p. 749-57.
167. Baron, A., et al., Fatty acid synthase: a metabolic oncogene in prostate cancer? J Cell Biochem, 2004. 91(1): p. 47-53.
168. Jensen, V., et al. The prognostic value of oncogenic antigen 519 expression and proliferative activity detected by antibody MIB-1 in node-negative breast cancer. J pathol, 1995. P. 176: 343-352.
169. Alo, P., et al. Expression of fatty acid synthase as a predictor of recurrence in stage I breast carcinoma patients. Cancer, 1996. 77: p. 474-482.
170. Wang, Y., et al. Fatty acid synthase expression in human breast cancer cell culture supernatants and in breast cancer patients. Cancer Lett, 2001. 167: p. 99-104.
171. Liu, B., et al. Triclosan inhibits enoyl-reductase of type I fatty acid synthase in vitro and is cytotoxic to MCF-7 and SKBr-3 breast cancer cells. Cancer Chemother Pharmacol, 2002. 49: p. 187-193.
172. Pizer, E., et al. Pharmcological inhibitors of mammalian fatty acid synthase suppress DNA replication and induce apoptosis in tumor cell lines. Cancer Res, 1998. 58: p. 4611-4615.
173. Menendez, J., et al. Antitumor actions of the anti-obesity drug orlistat in breast cancer cells: blockade of cell cycle progression, promotion of apoptotic cell death and PEA3- mediated transcriptional repression of Her2/neu oncogene. Ann Oncol, 2005. 16: p. 1253-1267.
174. Knowles, L., et al. A fatty acid synthase blockade induces tumor cell-cycle arrest by down-regulating Skp2. J Biol Chem, 2004. 279: 30540-30545.
175. Pizer, E., et al. Inhibition of fatty acid synthesis induces programmed cell death in human breast cancer cells. Cancer Res, 1996. 56: p. 2745-2747.
176. Menendez, J., et al. Inhibition of tumor-associated fatty acid synthase activity antagonizes estradiol- and tamoxifen- indued transactivation of estrogen-receptor in human endometrial adenocarcinoma cells. Oncogene, 2004. 23: p. 4945-4958.
177. Menendez, J., et al. RNA interference-mediated silencing of the p53 tumor-suppressor protein drastically increases apoptosis after inhibition of endogenous fatty acid metabolism in breast cancer cells. Int J Mol Med, 2005. 15: p. 33-40.
94
178. Kumar-Sinha, C., et al. Transcriptome analysis of HER2 reveals a molecular connection to fatty acid synthesis. Cancer Res, 2003. 63: p. 132-139.
179. Consolazio, A., et al., Overexpression of fatty acid synthase in ulcerative colitis. Am J Clin Pathol, 2006. 126(1): p. 113-8.
180. Li, J.N., et al.. Sterol regulatory element-binding protein-1 participates in the regulation of fatty acid synthase expression in colorectal neoplasia. Exp Cell Res, 2000. 261(1): p. 159-65.
181. Krontiras, H., et al., Fatty acid synthase expression is increased in neoplastic lesions of the oral tongue. Head Neck, 1999. 21(4): p. 325-9.
182. Menendez, J., et al. Fatty acid synthase and the lipogenic phenotype in cancer pathogenesis. Nature Reviews, 2007. 7: p. 763-777.
183. Priolo, C., et al. The isopeptidase USP2a regulates the stability of fatty acid synthase in prostate cancer. Cancer Res, 2006. 66: p. 8625-8632.
184. Lu, S, and Archer, MC. Sp1 coordinately regulates de novo lipogenesis and proliferation in cancer cells. Int J Cancer. 2009.
185. Zanetti, A., et al. Coordinate upregulation of Sp1 DNA-binding activity and urokinase receptor expression in breast carcinoma. Cancer Res, 2000. 60: p. 1546-1551.
186. Chiefari, E., et al. Increased expression of AP2 and Sp1 transcription factors in human thyroid tumors: a role in NIS expression regulation. BMC, 2002. 2: p. 35-38.
187. Shi, Q., et al. Constitutive Sp1 activity is essential for differential constitutive expression of vascular endothelial growth factor in human pancreatic adenocarcinoma. Cancer Res., 2001. 61(10): p. 4143-54.
188. Hosoi, Y., et al. Up-regulation of DNA-dependent protein kinase activity and Sp1 in colorectal cancer. Int J Oncol., 2004. 25: p. 461-468.
189. Abdelrahim, M., et al. Role of Sp proteins in regulation of vascular endothelial growth factor expression and proliferation of pancreatic cells. Cancer Res, 2004. 64: p. 6740- 6749.
190. Ishibashi, H., et al. Sp1decoy transfected to carcinoma cells suppresses the expression of vascular endothelial growth factor, transforming growth factor beta1, and tissue factor and also cell growth and invasion activities. Cancer Res, 2000. 60: p. 6531-6536.
191. Grinstein, E., et al. Sp1 as G1 cell cycle phase specific transcription factor in epithelial cells. Oncogene, 2002. 21: p. 1485-1492.
192. Chen, F., et al. Ectopic expression of truncated Sp1 transcription factor prolongs the S phase and reduces the growth rate. Anticancer Res, 2000. 20: p. 661-667.
193. Abdelrahim, M., et al. Small inhibitory RNA duplexes for Sp1 mRNA block basal and estrogen-induced gene expression and cell cycle progression in MCF-7 breast cancer cells. J Bio Chem, 2002. 277: p. 28815-28822.
95
194. Wang, L., et al. Transcription factor Sp1 expression is a significant predictor of survival in human gastric cancer. Clin Cancer Res, 2003. 9: p. 6371-6380.
195. Black, A., et al. Sp1 and krüppel-like factor family of transcription factors in cell growth regulation and cancer. J Cell Physiol. 2001. 188(2): p. 143-160.
196. Bae, I., et al. Signaling components involved in Bcl-w-induced migration of gastric cancer cells. Cancer Lett. 2009. 277(1): p. 22-28.
197. Rahman, K.M., et al. Indole-3-carbinol (I3C) induces apoptosis in tumorigenic but not in nontumorigenic breast epithelial cells. Nutr Cancer. 2003. 45(1):101-12.
198. Pappa, G., et al. Quantitative combination effects between sulforaphane and 3,3'- diindolylmethane on proliferation of human colon cancer cells in vitro. Carcinogenesis. 2007. 28(7): p. 1471-7.
199. Frydoonfar, H.R., McGrath, D.R., and Spigelman, A.D. Inhibition of proliferation of a colon cancer cell line by indole-3-carbinol. Colorectal Dis. 2002. 4(3): p. 205-207.
200. Bonnesen, C., et al. Dietary indoles and isothiocyanates that are generated from cruciferous vegetables can both stimulate apoptosis and confer protection against DNA damage in human colon cell lines. Cancer Res. 2001. 61(16): p. 6120-30.
201. Chinnakannu K, et al. Cell cycle-dependent effects of 3,3'-diindolylmethane on proliferation and apoptosis of prostate cancer cells. J Cell Physiol, 2009. 219: p. 94-9.
202. Smith S, et al. 3,3'-Diindolylmethane and genistein decrease the adverse effects of estrogen in LNCaP and PC-3 prostate cancer cells. J Nutr., 2008. 138(12): p. 2379-85.
203. Weng, J.R., et al. A potent indole-3-carbinol derived antitumor agent with pleiotropic effects on multiple signaling pathways in prostate cancer cells. Cancer Res., 2007. 67(16): p. 7815-24.
204. Hsu, J.C., Bjeldanes, L.F., Firestone, G.L., et al. Indole-3-carbinol mediated cell cycle arrest of LNCaP human prostate cancer cells requires the induced production of activated p53 tumor suppressor protein. Biochem Pharmacol. 2006. 72(12): p. 1714-23.
205. Kuang, Y.F. and Chen, Y.H. Induction of apoptosis in a non-small cell human lung cancer cell line by isothiocyanates is associated with P53 and P21. Food Chem Toxicol. 2004. 42(10): p. 1711-1718.
206. Leong, H., Firestone, G.L., and Bjeldanes, L.F. Cytostatic effects of 3,3'- diindolylmethane in human endometrial cancer cells result from an estrogen receptor- mediated increase in transforming growth factor-alpha expression. Carcinogenesis. 2001. 22(11): p. 1809-1817.
207. Mori, H., et al. Cell proliferation in cancer prevention; effects of preventive agents on estrogen-related endometrial carcinogenesis model and on an in vitro model in human colorectal cells. Mutat Res., 2001. 480-481: p. 201-207.
96
208. , E.P., et al. Extended treatment with physiologic concentrations of dietary phytochemicals results in altered gene expression, reduced growth, and apoptosis of cancer cells. Cancer Ther., 2007. 6(11): p. 3071-9.
209. Rahman, K.M., et al. Indole-3-carbinol (I3C) induces apoptosis in tumorigenic but not in nontumorigenic breast epithelial cells. Cancer., 2003. 45(1): p. 101-12.
210. Perez, E. and Muss, H. Optimizing adjuvant chemotherapy in early-stage breast cancer. Oncology, 2005. 19: p. 1759-1767.
211. Osborne, C., Wilson, P. and Tripathy, D. Oncogenes and tumor suppressor genes in breast cancer: potential diagnostic and therapeutic applications. Oncologist, 2004. 9: p. 361-377.
212. Wright, C., et al. Prognostic factors in breast cancer: immunohistochemical staining for Sp1 and NCRC 11 related to survival, tumor epidermal growth factor receptor and oestrogen receptor status. J Pathol, 1987. 153: p. 325-331.
213. Varshochi, R., et al. ICI182 induces p21Waf1 gene transcription through releasing histone deacetylase 1 and estrogen receptor alpha from Sp1 sites to induce cell cycle arrest in MCF-7 breast cancer cell line. J Bio Chem, 2005. 280: p. 3185-3196. 214. Zanetti, A., et al. Inhibition of Sp1 activity by decoy PNA-DNA chimera prevents urokinase receptor expression and migration of breast cancer cells. Biochem Pharmacol, 2005. 70: p. 1277-1287. 215. Chadalapaka, G., et al. Curcumin decreases specificity protein expression in bladder cancer cells. Cancer Res., 2008. 68(13): p. 5345-5354.