Tumour-Stroma Signalling in Cancer Cell Motility and Metastasis
by
Valbona Luga
A thesis submitted in conformity with the requirements for the degree of Doctor of Philosophy,
Department of Molecular Genetics, University of Toronto
© Copyright by Valbona Luga, 2013
Tumour-Stroma Signalling in Cancer Cell Motility and Metastasis
Valbona Luga
Doctor of Philosophy
Department of Molecular Genetics University of Toronto
2013
Abstract
The tumour-associated stroma, consisting of fibroblasts, inflammatory cells, vasculature and extracellular matrix proteins, plays a critical role in tumour growth, but how it regulates cancer cell migration and metastasis is poorly understood. The Wnt-planar cell polarity (PCP) pathway regulates convergent extension movements in vertebrate development. However, it is unclear whether this pathway also functions in cancer cell migration. In addition, the factors that mobilize long-range signalling of Wnt morphogens, which are tightly associated with the plasma membrane, have yet to be completely characterized. Here, I show that fibroblasts secrete membrane microvesicles of endocytic origin, termed exosomes, which promote tumour cell protrusive activity, motility and metastasis via the exosome component Cd81. In addition, I demonstrate that fibroblast exosomes activate autocrine Wnt-PCP signalling in breast cancer cells as detected by the association of Wnt with Fzd receptors and the asymmetric distribution of
Fzd-Dvl and Vangl-Pk complexes in exosome-stimulated cancer cell protrusive structures.
Moreover, I show that Pk expression in breast cancer cells is essential for fibroblast-stimulated cancer cell metastasis. Lastly, I reveal that trafficking in cancer cells promotes tethering of autocrine Wnt11 to fibroblast exosomes. These studies further our understanding of the role of ii the tumour-associated stroma in cancer metastasis and bring us closer to a more targeted approach for the treatment of cancer spread.
iii
Acknowledgements
My journey as a PhD student has been an amazing learning experience. This would not have been possible without a number of people who were there for me to share both the challenges and rewards of my scientific endeavours.
Jeff, it has been an honour and privilege to be your student. I am deeply grateful to you for believing in me and helping me realize that science is my call in life. Your passion, brilliance and mastery of science will always be an inspiration to me.
Lil, thank you for your support and advice. You are an important role model to me and I am very grateful for your mentorship.
Thanks to my committee members, Dr. Igor Jurisica, Dr. David Kaplan and Dr. Rama Khokha, for their suggestions and support.
Thank you to all the past and current members of the Wrana and Attisano labs. I spent the last nine years of my life mainly in the lab and many of you became my friends and family. John, thank you for your mentorship during my first year in the lab when I barely knew about science. Christine, thank you for teaching me as a young student, aka your “little One”, how to properly design and carry out experiments. You are a remarkable scientist and I am particularly proud to be your friend. Miriam, I will always be thankful to you for your support and encouragment during my search for the “Luga factors”. Your wisdom and advice have been greatly helpful to me throughout my PhD career. I deeply cherish our friendship and will sorely miss our laughs. Abi, thanks for being a good friend and I will miss our chats by the phosphoimager. Liang, thank you for your help; it was a pleasure working with you. Alicia, thank you for your help and friendship. To everyone else, thank you for your support and friendship. I will miss all of you.
To my family, thank you for your unconditional love and helping me become the person I am today. Dad, you taught me to dream big and believe in myself. Rovi, your intelligence, talent and search for perfection have been deeply inspirational to me. Koli, your bigheartedness and sense of justice are your best virtues and I look up to you for that. Calvin, Jason, Brandon, Laetitia and Delora, I thank you for bringing pure joy to my life. Mom, your love and devotion
iv to your children is unparalleled. You taught me early in my life to work hard and be thorough; these lessons served me well during my PhD. I dedicate this thesis to you.
Finally, Rohit, thank you for being by my side for the last eleven years. Your wisdom, patience and love have been crucial for my professional and personal growth. Words cannot express my gratitude and love for you and I look forward to our life journey together.
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Table of Contents
Abstract ...... ii
Acknowledgements ...... iv
Table of Contents ...... vi
List of Figures and Tables ...... ix
List of Abbreviations and Symbols ...... x
Chapter 1 : General Introduction ...... 1 1.1. Cell Motility and Cancer ...... 2 1.1.1. Overview of cancer hallmarks ...... 2 1.1.2. Autonomous cancer hallmarks ...... 2 1.1.3. Neovascularization and suppression of the immune system ...... 5 1.1.4. Apical-basolateral cell polarity as a barrier to tumour cell invasiveness ...... 8 1.1.5. Tumour cell migration ...... 12 1.1.6. Metastasis – colonization of distant organs ...... 22 1.1.7. The tumour microenvironment ...... 27 1.1.8. Fibroblasts as components of the tumour microenvironment ...... 30 1.1.9. Identification and function of cancer stem-like cells ...... 32 1.2. Noncanonical Wnt-Planar Cell Polarity Pathway ...... 33 1.2.1. Planar cell polarity and its manifestations ...... 33 1.2.2. Molecular PCP components in the fly ...... 36 1.2.3. Models of PCP signalling in the fly ...... 37 1.2.4. PCP signalling in vertebrates ...... 39 1.2.5. Wnt structure and post-translational modifications ...... 44 1.2.6. Wnt signalling pathways ...... 46 1.2.7. Role of PCP in cell motility and cancer ...... 49 1.3. Exosomes as Potent Mediators of Intercellular Communication ...... 50 1.3.1. Modes of intercellular communication ...... 50 1.3.2. Introduction to exosomes ...... 50 1.3.3. Exosome biogenesis ...... 51 1.3.4. Exosome components ...... 54 1.3.5. Exosome functions ...... 55 1.3.6. Exosomes as biomarkers for disease ...... 57 1.3.7. Exosomes as therapeutic tools ...... 57 vi
1.3.8. Tetraspanins – masters of multiple biological functions ...... 58 1.3.9. Cd81 – an exemplary tetraspanin ...... 63 1.4. Overview of Thesis ...... 67
Chapter 2 : Fibroblast-secreted Exosomes Regulate Breast Cancer Cell Motility and Metastasis ...... 69 2.1. Introduction ...... 70 2.2. Materials and Methods ...... 71 2.2.1. Cell Culture ...... 71 2.2.2. Conditioned Media Preparation ...... 72 2.2.3. Single Cell Motility Assay ...... 72 2.2.4. 3D Matrigel Cultures ...... 73 2.2.5. Orthotopic Mouse Model of Breast Cancer Metastasis ...... 73 2.2.6. Immunohistochemistry ...... 73 2.2.7. Protein Chromatography ...... 74 2.2.8. Mass Spectrometry ...... 75 2.2.9. Exosome Isolation By Differential Ultracentrifugation ...... 76 2.2.10. Electron Microscopy ...... 76 2.2.11. Exosome Purification by Sucrose Gradient Ultracentrifugation ...... 77 2.2.12. Methyl-β-Cyclodextrin (MβCD) Treatment ...... 77 2.2.13. Exosome Immuno-Magnetic Extraction ...... 77 2.2.14. Immunoblotting ...... 78 2.2.15. RNA Extraction and Real-Time Quantitative PCR (RT-qPCR) ...... 78 2.2.16. PCR Primer Sets ...... 79 2.2.17. Cell Transfection ...... 79 2.2.18. shRNA Sequences ...... 80 2.2.19. Cell Lysis ...... 80 2.2.20. Analysis of Human Stroma Gene Expression Data ...... 81 2.3. Results ...... 81 2.3.1. L cell-secreted Factors Stimulate Breast Cancer Cell Protrusive Activity and Motility ...... 81 2.3.2. L cell-secreted Factors Stimulate Breast Cancer Cell Invasiveness and Metastatic Potential 86 2.3.3. Identification and Characterization of L cell-secreted Exosomes ...... 90 2.3.4. Functional Characterization of L cell-secreted Exosomes ...... 104 2.3.5. Cd81 Functions As a Component of L cell-secreted Exosomes to Promote BCC Motility .... 107 2.3.6. Cd81 Is Necessary For L cell-stimulation of BCC Metastasis ...... 110 2.3.7. Human CAFs Secrete Cd81-positive Exosomes That Stimulate BCC Motility ...... 113 2.4. Discussion ...... 115
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Chapter 3 : Fibroblast Exosomes Mobilize the Wnt-PCP Pathway to Promote Breast Cancer Cell Motility and Metastasis ...... 118 3.1. Introduction ...... 119 3.2. Materials and Methods ...... 120 3.2.1. Cell Culture ...... 120 3.2.2. Conditioned Media Preparation ...... 120 3.2.3. Single Cell Motility Assay ...... 121 3.2.4. Cell Transfection ...... 121 3.2.5. shRNA Sequences ...... 121 3.2.6. Cell Lysis And Immunoblotting ...... 122 3.2.7. RNA Extraction and Real-Time Quantitative PCR (RT-qPCR) ...... 122 3.2.8. PCR Primers ...... 123 3.2.9. Immunofluorescence ...... 124 3.2.10. L cell / MDA-MB-231 Orthotopic Mouse Model of Breast Cancer Metastasis ...... 124 3.2.11. DNA Constructs ...... 125 3.2.12. Exosome Isolation by Differential Ultracentrifugation ...... 125 3.2.13. Exosome Internalization Assay: Immunoprecipitation ...... 125 3.2.14. Exosome Internalization Assay: Immunofluorescence and Dynasore Treatment ...... 126 3.2.15. Electron Microscopy ...... 126 3.2.16. Exosome Immuno-Magnetic Extraction ...... 126 3.3. Results ...... 127 3.3.1. Core PCP Components Mediate Fibroblast-Induced BCC Protrusive Activity and Motility ... 127 3.3.2. Pk1 Expression Is Necessary For L cell-Stimulated BCC Metastasis ...... 131 3.3.3. Core PCP Components Distribute Asymmetrically in ACM-treated BCCs ...... 134 3.3.4. Autocrine Wnts Mediate Fibroblast-Induced BCC Protrusive Activity and Motility ...... 141 3.3.5. Fibroblast Exosomes Mobilize Autocrine Wnt-PCP Signalling in BCCs ...... 147 3.4. Discussion ...... 157
Chapter 4 : Thesis Summary and Future Directions ...... 160 4.1. Overview ...... 161 4.2. Unanswered Questions and Future Directions ...... 163
References ...... 168
Copyright Acknowledgment ...... 192
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List of Figures and Tables
Figure 1.1 The Tumour-associated Stroma Influences Tumour Growth ...... 7 Figure 1.2 Apical-Basal Polarity in Epithelial Cells ...... 11 Figure 1.3 Remodelling of the Actin Cytoskeleton ...... 14 Figure 1.4 Cell Migration As a Multistep Process ...... 18 Figure 1.5 The Metastatic Cascade ...... 26 Figure 1.6 PCP in Drosophila and Vertebrates ...... 42 Figure 1.7 Wnt Signalling Pathways ...... 48 Figure 1.8 Schematic Structure of Cd81 As a Prototypical Tetraspanin ...... 61 Figure 1.9 Cd81 and Tetraspanin-Enriched Microdomains (TEMs) ...... 64 Figure 2.1 L cell-secreted Factors Stimulate BCC Protrusive Activity and Motility ...... 83 Figure 2.2 ACM Promotes Protrusive Activity and Motility in Several BCCs ...... 85 Figure 2.3 L cell-secreted Factors Promote MDA-MB-231 Invasiveness and Metastasis ...... 88 Figure 2.4 Fractionation of ACM by Protein Chromatography ...... 91 Table 2-1 Proteins in Fraction Q3 Identified by Mass Spectrometry ...... 93 Figure 2.5 The Active Fractions of ACM Contain Exosomes ...... 102 Figure 2.6 L cell-secreted Exosomes Activate MDA-MB-231 Cell Motility ...... 105 Figure 2.7 Cd81 Functions As a Component of Exosomes ...... 108 Figure 2.8 Cd81 Is Necessary For L cell-stimulated BCC Metastasis ...... 111 Figure 2.9 Human CAFs Secrete Cd81-positive Exosomes That Stimulate BCC Motility ...... 114 Figure 3.1 Core PCP Components Mediate ACM Activity in BCCs ...... 129 Figure 3.2 Prickle1 Is Required For L cell-stimulated MDA-MB-231 Cell Metastasis ...... 132 Figure 3.3 Localization of Fzd6-Dvl1 Complexes in ACM-treated MDA-MB-231 Cells ...... 136 Figure 3.4 Pk1 and Vangl1 Localize Asymmetrically in ACM-treated MDA-MB-231 Cells ...... 137 Figure 3.5 Localization of Fzd7-Dvl3 Complexes in ACM-stimulated SUM-159PT Cells ...... 139 Figure 3.6 Fzd6-Dvl1 Complexes Localize Asymmetrically in Exosome-stimulated BCCs ...... 140 Figure 3.7 Porcupine Expression Is Necessary in BCCs ...... 143 Figure 3.8 BCC-produced Wnt11 Is Necessary For ACM Activity ...... 145 Figure 3.9 BCCs Are Deficient For Cd81-positive Exosomes ...... 148 Figure 3.10 MDA-MB-231 Cells Internalize L cell-secreted Exosomes ...... 150 Figure 3.11 Wnt11 Associates With L cell Exosomes Upon Trafficking In BCCs ...... 154 Figure 3.12 A Model For Fibroblast Exosomes Stimulating Wnt-PCP Signalling In BCCs ...... 156
ix
List of Abbreviations and Symbols
α alpha β beta γ gamma µ micro
AB apicobasal polarity ACM active conditioned media ADAM a disintegrin and metalloproteinase AP anteroposterior APC adenomatous polyposis coli aPKC atypical protein kinase C Arp2/3 actin related proteins 2 and 3
BCC breast cancer cell BMP bone morphogenetic protein
CAF cancer-associated fibroblast CCL CC chemokine ligand Cd81 cluster of differentiation 81 Cdc42 cell division control protein 42 homolog CE convergent extension Celsr cadherin EGF LAG seven-pass G-type receptor Ck1 casein kinase 1 CRB crumbs CRD cysteine-rich domain CSC cancer stem-like cells CTD carboxy-terminal domain
Dgo diego DLG discs-large homologue DNA deoxyribonucleic acid Dsh dishevelled (fruit fly) DV dorsoventral Dvl dishevelled (vertebrates)
ECM extracellular matrix EGF epidermal growth factor EGFR epidermal growth factor receptor ERM ezrin-radixin-moesin EM electron microscopy EMT epithelial-to-mesenchymal transition x
ESCRT Endosomal Sorting Complex Required for Transport EWI glutamate-tryptophan-isoleucine
F-actin filamentous actin FAK focal adhesion kinase FGF fibroblast growth factor Fmi flamingo Fz frizzled receptor (fruit fly) Fzd frizzled receptor (vertebrate)
GAP GTPase activating protein GEF guanine nucleotide exchange factor GSK3β glycogen synthase kinase 3 beta GTPase guanosine triphosphatase
HGF hepatocyte growth factor
ICAM intercellular-adhesion molecule IGF insulin growth factor Igsf8 immunoglobulin superfamily member 8 IL interleukin
JNK c-Jun N-terminal kinase
LEL large extracellular loop LR left-right LRP lipoprotein receptor-related protein
MET mesenchymal-to-epithelial transition MHC major histocompatibility complex miRNA microRNA ML mediolateral MLC myosin light-chain MLCK myosin light-chain kinase MMP matrix metalloproteinase MS mass spectrometry MT microtubule MVB multivesicular body Myc myelocytomatosis viral oncogene homolog
NK natural killer cell NTD amino-terminal domain
xi
PAK Gβγ/p21-activated kinase 1 PAR partitioning defective PCP planar cell polarity PDGF platelet derived growth factor PDGFRβ platelet derived growth factor receptor beta PI3K phosphoinositide 3-kinase Pk prickle PKC protein kinase C PTEN phosphatase and tensin homolog Ptgfrn prostaglandin F2 receptor negative regulator p53 tumour protein p53
Rab member Ras oncogene family Ras rat sarcoma viral oncogene homolog Rac1 Ras-related C3 botulinum toxin substrate 1 RET receptor tyrosine kinase RNA ribonucleic acid RhoA ras homolog family member A ROCK Rho kinase Ryk Receptor-like tyrosine kinase
SCRIB scribble homologue SDF stromal cell-derived factor Sf Smurf siRNA small interfering RNA SMA smooth muscle actin Smad mothers against decapentaplegic homolog Smurf Smad ubiquination regulatory factor Src sarcoma viral oncogene homolog
TEM tetraspanin-enriched membrane TGFβ transforming growth factor beta TGFβRI transforming growth factor beta receptor I TGFβRII transforming growth factor beta receptor II TIAM-1 T-cell lymphoma invasion and metastasis-1 TNFα tumour necrosis factor α
Vang van Gogh Vangl vang-like VEGF vascular endothelial growth factor
WASP Wiskott-Aldrich syndrome protein WAVE WASP family verprolin-homology protein Wg wingless Wls wntless xii
Chapter 1 : General Introduction
1
1.1. Cell Motility and Cancer
1.1.1. Overview of cancer hallmarks
Cancers arise from cells with genomic aberrations, which provide the genetic diversity that is necessary to drive malignancy (Hanahan and Weinberg, 2011; Talmadge and Fidler, 2010). All cancers share universal characteristics, or hallmarks, that provide self-sufficiency in growth signals, insensitivity to anti-growth signals, resistance to cell death, limitless replicative potential, reprogramming of energy metabolism, induced angiogenesis, evasion of attack from the immune system and activation of invasion and metastasis (Hanahan and Weinberg, 2011).
Importantly, these hallmarks are interconnected as, for example, major oncogenes and tumour suppressor genes that influence cell proliferation also affect cell survival, cell metabolism, cell motility, angiogenesis and evasion of the immune system (Hanahan and Weinberg, 2011;
Koppenol et al., 2011; Mantovani et al., 2008). Also, a very important conceptual progress in the field of cancer research has been the recognition that cancer biology is tightly regulated by the surrounding stroma (Bissell and Hines, 2011).
1.1.2. Autonomous cancer hallmarks
Tumour growth is facilitated by a series of distinct and complementary events that occur within cancer cells (Hanahan and Weinberg, 2011; Talmadge and Fidler, 2010). Continuous proliferative signalling is thought to be one of the earliest hallmarks acquired by cancer cells
(Hanahan and Weinberg, 2011; Talmadge and Fidler, 2010). Normally, tissues maintain their characteristic architecture and function by tightly regulating the production of growth-promoting signals, consisting typically of growth factors, which instruct growth and division in
2
neighbouring cells in a temporally and spatially organized fashion (Lemmon and Schlessinger,
2010; Witsch et al., 2010). Cancer cells acquire the ability to sustain proliferative signalling independently of the cues provided by their neighbouring cells. They do so via several mechanisms, including elevated self-production of growth factors (GFs) (such as epidermal GF
(EGF) and insulin-like GF (IGF) (Witsch et al., 2010), co-option of normal cells in the tumour microenvironment to produce growth signals that in turn act on cancer cells (Kalluri and
Zeisberg, 2006), upregulation of expression of growth factor receptors (such as EGF receptor
(EGFR)) (Lemmon and Schlessinger, 2010), or acquisition of oncogenic mutations that lead to constitutive activation of growth factor receptors (such EGFR, platelet-derived GF receptor
(PDGFR), fibroblast GF receptor (FGFR)) (Lemmon and Schlessinger, 2010) or downstream effectors (such as rat sarcoma viral oncogene homolog (Ras) and myelocytomatosis viral oncogene homolog (Myc)) (Dang, 2012; Karnoub and Weinberg, 2008) that in turn signal uncontrolled cancer cell proliferation (Hanahan and Weinberg, 2011). Tissue homeostasis is also maintained by growth inhibitory signals, including transforming growth factor beta (TGFβ)
(Massague, 2012) and phosphatase and tensin homolog (PTEN) (Song et al., 2012), and cellular programs, such as cell senescence (Collado and Serrano, 2010; Nardella et al., 2011) and contact inhibition (Martin-Belmonte and Perez-Moreno, 2012), which tumour cells must disable in order to proliferate excessively. TGFβ signals through the TGFβ type 1 and type 2 serine- threonine kinase receptors (TβRI and TβRII respectively), which activate the receptor-regulated
Smad proteins (Smad2/3) that in a complex with common partner Smad (Smad4) mediate
TGFβ-induced expression of several cell cycle inhibitory factors and inhibition of cell proliferation factors (Attisano and Wrana, 2002; Massague, 2012). Indeed, TβRII and Smad4 are commonly inactivated through mutation and loss of heterozygosity in various cancers
(Attisano and Wrana, 2002; Massague, 2012). Other tumour suppressor genes, such as merlin 3
and liver kinase B1 (LKB1), which regulate contact inhibition of cell proliferation, are also commonly inactivated in many cancers (Li et al., 2012a; Martin-Belmonte and Perez-Moreno,
2012). Next, cancer cells overcome senescence, which is a cellular program that is normally activated once the cells have undergone a limited number of successive cell growth and division cycles (Collado and Serrano, 2010; Nardella et al., 2011) and is controlled by tumour protein p53 (p53) and retinoblastoma-associated (RB) proteins (Polager and Ginsberg, 2009). Cellular senescence prevents genomic instability due to end-to-end fusion of chromosomes with eroded telomeres (Collado and Serrano, 2010; Harley, 2008; Nardella et al., 2011). Initially, cancer cells use the unprotected ends of chromosomes as a means to generate genomic instability, which leads to activation of oncogenes and suppression of tumour-suppressor genes (Campbell,
2012; Harley, 2008). Then, cancer cells acquire the ability to express telomerase, a specialized
DNA polymerase that adds telomere repeat segments to the ends of telomeric DNA, and consequently attain replicative immortality (Campbell, 2012; Hanahan and Weinberg, 2011;
Harley, 2008). Furthermore, cancer cells must resist programmed cell death, which is another line of defence against hyperproliferation and genomic instability. Cancer cells manipulate potent cellular programs, including apoptosis, autophagy and necrosis, which are carried out by a myriad of regulatory (p53, B-cell CLL/Lymphoma (Bcl) proteins, Beclin-1) and effector
(caspases 8) components, in order to attenuate cell death and ensure their survival (Giansanti et al., 2011; Kreuzaler and Watson, 2012). Finally, cancer cells also reprogram their glucose metabolism to carry out aerobic glycolysis, a phenomenon known as the Warburg effect, which is thought to divert intermediates for nucleotide and amino acid biosynthesis that in turn act as building blocks for cell growth and proliferation (Koppenol et al., 2011).
4
1.1.3. Neovascularization and suppression of the immune system
Tumour cells must also interact with normal cells to direct neovascularization and inflammation, which support tumour growth (Folkman, 2007; Hanahan and Weinberg, 2011; Mantovani et al.,
2008) (Figure 1.1A). Tumours demand a constant supply of nutrients, O2/CO2 gas exchange as well as removal of metabolic waste. To fulfill this requirement, tumour cells stimulate new blood vessel formation via angiogenesis (Folkman, 2007), a process whereby endothelial cells are recruited and assemble new blood vessels branching from existing ones, or vasculogenesis, a process whereby bone-marrow derived cells produce endothelial cells that assemble into new vessels (Lyden et al., 2001). Tumour cells switch on this processes by producing angiogenic factors, such as the vascular endothelial growth factors (VEGFs), fibroblast growth factors
(FGFs) and angiopoietin 2 (ANGPT2), which act on endothelial cells or bone marrow-derived cells to instruct new blood vessel growth (Folkman, 2007) (Figure 1.1B). Cancer cells also inhibit the production of anti-angiogenic factors, such as endostatin and thrombospondin 1
(TSP-1), that impede the induction of angiogenesis (Folkman, 2007). Tumour blood vessels have aberrant characteristics, in that they sprout and convolute excessively and have erratic blood flow, and are conducive to malignancy due to deficiency in pericytes, which normally prevent the endothelial wall from being leaky (Hanahan and Weinberg, 2011). Cancer cells also secrete VEGF-C and VEGF-D to stimulate lymphangiogenesis, the process of new lymphatic vessel formation from lymphatic endothelial cells (Tammela and Alitalo, 2010). The lymphatic system plays a critical role in tumour dissemination and metastasis and the density of lymphatic vessels correlates with the incidence of lymph node metastasis and poor prognosis (Tammela and Alitalo, 2010).
5
Cancer cells also participate in a complex dialogue with cells of the immune system, which acts to both abolish and stimulate tumourigenesis (Mantovani et al., 2008). Studies have shown that the adaptive immune system carries out surveillance and attacks nascent tumours (Mantovani et al., 2008). However, tumours cells acquire the ability to evade the adaptive immune system by several mechanisms, including the secretion of immunosuppressive factors, such as interleukin-
10 (IL-10) and TGFβ, and recruitment of inflammatory cells, including macrophages with an
M2 phenotype, neutrophils and mast cells, as well as distinct subclasses of cells of the adaptive immune system, such as T helper 2 (TH2) cells and certain B lymphocytes that suppress the activity of cytotoxic lymphocytes (Mantovani et al., 2008) (Figure 1.1A). Activation of oncogenes, such as Ras, Myc and receptor tyrosine kinase (RET), and inactivation of tumour suppressor genes, such as TGFβRII, in tumour cells, leads to induction of a transcriptional program that drives the expression of several chemokines (such as CC-chemokine ligand 2
(CCL2) and CCL20), cytokines (such as IL-1β, IL-6, IL-23 and tumour necrosis factor α
(TNFα)) and prostaglandins that recruit inflammatory cells to the tumour microenvironment
(Mantovani et al., 2008) (Figure 1.1B). Importantly, inflammatory cells secrete chemicals, such as reactive oxygen and nitrogen species, which can damage DNA and accelerate genetic aberrations that induce malignancy (Mantovani et al., 2008). In fact, clinical studies indicate that inflammation arising from microbial infections or autoimmune diseases increase the risk of developing cancer and that therapy with non-steroidal anti-inflammatory agents decrease the incidence of mortality from different tumours (Mantovani et al., 2008). In addition, inflammatory cells produce growth factors, chemokines, cytokines and metalloproteases that amplify the inflammatory response, induce angiogenesis and lymphangiogenesis, remodel the
ECM and promote tumour cell survival, migration, invasion and metastasis (Mantovani et al.,
2008). 6
A Epithelial Cell Cancer Cell (CC)
Basement Cancer-Associated Membrane Fibroblast (CAFs) Inflammatory Cells (ICs)
Extracellular Bone Marrow Derived Matrix (ECM) Stem & Progenitor Cells (BMDCs)
Endothelial Lymphatic Cell (EC) Endothelial Motile & Cell (LEC) Invasive Cancer Pericyte Cell (MCC) B
TGF MMPs HGF ROS FGF2 TGF CSF EGF EGF SDF-1 TNF Tenascin C IL-1 VEGF-C CCL5 VEGF-D CCL21 VEGF FGF ANGPT2
Figure 1.1 The Tumour-associated Stroma Influences Tumour Growth
(A) Tumour progression is supported by several stromal cells, including cancer-associated fibroblasts (CAFs), bone marrow-derived cells (BMDCs) and inflammatory cells (ICs), and vasculature cells (blood and lymphatic). (B) Cancer cells (CCs) communicate with stromal cells by numerous secreted factors. For instance, CCs secrete factors that activate CAFs, which in turn remodel ECM and promote CC invasiveness. Moreover, CCs secrete several factors that induce angiogenesis (by recruiting endothelial cells (ECs) or BMDCs) or lymphangiogenesis (by recruiting lymphatic ECs (LECs)) within the tumour. The new vasculature provides 7
nutrients and removes metabolic waste. Further, CCs recruit ICs, including macrophages, neutrophils and mast cells, which promote tumour growth, CC invasiveness and activate angiogenesis. ICs also secrete factors that inhibit immune cells, such as cytotoxic T cells and dendritic cells (not shown), which destroy tumour cells.
1.1.4. Apical-basolateral cell polarity as a barrier to tumour cell invasiveness
Although tumour growth can be detrimental to patient health, it is metastasis, the process of spreading and growth of tumours in secondary organs, that accounts for approximately 90% of cancer-associated mortality (Talmadge and Fidler, 2010). In order to disseminate in distant tissues, cancer cells must first detach from the primary tumour and invade the surrounding environment. In the case of epithelial cells, acquisition of an invasive phenotype involves loss of apical-basolateral (AB) cell polarity and cell-cell adhesions, alteration in cell shape, and increased cell motility (Martin-Belmonte and Perez-Moreno, 2012; Thiery et al., 2009) (Figure
1.2). Normal epithelium exists as a single layer of cells attached to each other via cell-cell junctions, including tight junctions, adherens junctions and desmosomes, which form within lateral membranes (Martin-Belmonte and Perez-Moreno, 2012; Thiery et al., 2009) (Figure 1.2).
Also, epithelial cells attach to the underlying basement membrane via integrins in their basal membrane and face the luminal space or the external environment via their apical membrane.
Epithelial cells exhibit apical-basolateral polarity, which is characterized by asymmetric distribution of cellular components, such as proteins and lipids, and organelles along the AB axis (Martin-Belmonte and Perez-Moreno, 2012) (Figure 1.2). Crosstalk between cell adhesions
(tight junctions, which are comprised of transmembrane proteins occludin, claudin and junctional adhesion molecule (JAM), and cytoplasmic proteins zonula occludens (ZO) 1-3, and
8
adherens junctions, which are comprised of two adhesive complexes: cadherin-catenins (p-120 catenin, α-catenin and β-catenin) and nectin-afadin) and three triprotein polarity complexes (the partitioning-defective 3 (PAR3)-PAR6-atypical protein kinase C (aPKC) complex, the transmembrane protein crumbs (CRB)-protein associated with lin-seven (PALS)-PALS1- associated tight-junction protein (PATJ) complex and the scribble homologue (SCRIB)-lethal
(2) giant larvae homologue (LGL)-discs-large homologue (DLG) complex) is critical for the establishment and maintenance of AB polarity (Martin-Belmonte and Perez-Moreno, 2012;
Thiery et al., 2009) (Figure 1.2). The PAR6 polarity complex promotes the establishment of the apical-basal membrane border as it is a critical regulator of tight-junctions (Ozdamar et al.,
2005), the CRB complex is required for the establishment of the apical membrane and the
SCRIB complex defines the basolateral plasma domain (Martin-Belmonte and Perez-Moreno,
2012). In addition, cell adhesion proteins and polarity complexes connect to microtubules and the actin cytoskeleton to regulate cell shape and polarity (Iden and Collard, 2008; Martin-
Belmonte and Perez-Moreno, 2012; Thiery et al., 2009). Moreover, cell-cell adhesion proteins and polarity complexes crosstalk with signalling pathways such as TGFβ, Wnt, Hedgehog and
Hippo pathways and mechanistic target of rapamycin serine/threonine kinase (mTOR)- dependent energy metabolism to control cell polarity, adhesion, growth, proliferation, differentiation and cell death (Martin-Belmonte and Perez-Moreno, 2012; Thiery et al., 2009).
AB polarity is a critical barrier to the formation of carcinoma, which is cancer of epithelial origin that accounts for the most prevalent form of malignancy in humans. Misregulation of expression and/or function of the protein components that comprise cell adhesions and polarity complexes, results in breakage of intercellular adhesions, loss of polarized characteristics of
9
epithelial cells, hyperproliferation and acquisition of migratory and invasive potential (Martin-
Belmonte and Perez-Moreno, 2012; Thiery et al., 2009). Loss of AB cell polarity is closely associated with epithelial-to-mesenchymal transition (EMT), a developmentally regulatory program whereby epithelial cells lose their differentiated characteristics and acquire mesenchymal characteristics through activation of a transcriptional program, which represses the expression of several polarity proteins and induces the expression of other proteins necessary for the mesenchymal phenotype (Thiery et al., 2009). TGFβ signalling through
Smad-dependent and Smad-independent pathways plays a pivotal role in AB cell polarity and
EMT (Barrios-Rodiles et al., 2005; Heldin et al., 2012; Ozdamar et al., 2005; Varelas et al.,
2010) (Figure 1.2). Occludin interacts with and restricts the localization of TβRI at tight junctions, where the receptor associates constitutively with Par6 (Barrios-Rodiles et al., 2005).
Upon TGFβ binding to the TβRI/TβRII receptor complex, TβRII phosphorylates Par6, which then associates with the Smad ubiquitination regulator factor-1 (Smurf1) that in turn targets the guanosine triphosphatase RhoA for degradation, thereby leading to loss of tight junctions
(Ozdamar et al., 2005). In addition, TGFβ signalling through the Smad pathway, directly activates expression of EMT-inducing transcription factors, such as Snail and Twist, which repress the expression of several proteins required for AB polarity, including E-catherin, Par3 and Crumbs (Heldin et al., 2012; Thiery et al., 2009). Moreover, TGFβ influences the activity of several other signalling pathways, including Notch, Wnt and integrin signalling, which also trigger EMT (Heldin et al., 2012; Thiery et al., 2009). Importantly, TGFβ signalling is controlled by the Hippo pathway members, WW domain containing transcription regulator 1
(Taz) and Yes-associated protein (Yap), which sequester Smad2/3 and are coupled to the
Crumbs polarity complex, thus suppressing TGFβ signalling at high cell densities (Varelas et al., 2010). Loss of AB cell polarity and cell-cell adhesions and acquisition of a mesenchymal 10
phenotype, including enhanced migratory potential and upregulation of ECM-remodelling metalloproteinases, allows cancer cells to detach from the primary tumour and invade the surrounding tissue (Thiery et al., 2009).
Luminal Space
-
Apical F-actin PATJ CRB PALS JAM Microtubule Claudin ZO3 Golgi Occludin ZO2 Tight ZO1 TIAM1 Rac1 junction PAR6 aPKC RhoA T RI PAR3 Cdc42 Nectin Afadin
Lateral Adherens Nucleus E-catherin -cat -actinin -cat junction p120 Desmocollin Desmoglein DLG Desmosomes Integrins SCRIB LGL Connexin Gap + junction Basal
Basement Membrane
Figure 1.2 Apical-Basal Polarity in Epithelial Cells
Epithelial cells are polarized along the apical-basal (AB) axis as detected by the orientation of cellular organelles (including the nucleus, Golgi and microtubules (MTs)), and asymmetrical distribution of lipids (not shown) and proteins (such as cell junction components). The epithelium is held together by cell-cell adhesions, comprised of tight junctions (green), adherens junctions (aquamarine), desmosomes (blue) and gap junctions (grey), and is attached to the basement membrane via cell-matrix adhesions mediated by integrins (yellow). Tight junctions are localized at the border of apical and basolateral domains and hinder the movement of proteins and lipids between these membranes. Both tight junctions and adherens junctions
11
together with the polarity complexes: CRB (components indicated in deep blue), PAR6 (components indicated in deep purple) and SCRIB (components indicated in deep orange) establish and maintain AB polarity. The polarity complexes function by antagonizing each other: the CRB and the PAR6 complexes establish the apical-lateral border while the SCRIB complex establishes the lateral-basal border. Also, tight junction and adherens junction components and polarity proteins interact with MTs (p120 catenin and PAR6; not shown) and/or the actin cytoskeleton components (shown in red) to regulate cell shape and polarity. TGFβ receptor type I (TβRI) interacts with occludin and PAR6 and regulates tight junction maintenance in response to TGFβ signalling. Figure adapted from (Martin-Belmonte and Perez- Moreno, 2012; Thiery and Sleeman, 2006).
1.1.5. Tumour cell migration
Acquisition of a migratory phenotype is critical for tumour cell invasive and metastatic capacity
(Friedl and Alexander, 2011; Nurnberg et al., 2011). Cell migration is facilitated primarily by the actin cytoskeleton, which consists of polymerized actin, also known as filamentous actin (F- actin), and several actin-binding proteins that regulate the rate and organization of actin polymerization (Campellone and Welch, 2010; Pollard, 2007; Ridley et al., 2003) (Figure 1.3).
Actin filaments are structurally polarized and grow rapidly at the plus end and slowly at the minus end (Campellone and Welch, 2010; Ridley et al., 2003). Actin nucleation factors, such as formins and the actin-related protein 2/3 (Arp2/3) complex stimulate actin filament elongation and branching respectively, while capping proteins, such as gelsolin, halt filament elongation by binding to the plus end of F-actin (Campellone and Welch, 2010; Pollard, 2007). Other actin- binding proteins regulate the pool of available actin by either binding actin monomers (such as profilin) or disassembling older filaments (such as members of the actin depolymerization factor
12
(ADF)/cofilin family) (Campellone and Welch, 2010; Pollard, 2007; Ridley et al., 2003).
Furthermore, cortactin proteins stabilize new branches while filamin A and α-actinin stabilize the whole cytoskeleton by cross-linking F-actin (Pollard, 2007; Ridley et al., 2003). In response to extracellular stimuli, the Rho (Ras homologous) family of small guanosine triphosphate
(GTP)-binding proteins, including Cdc42, Rac and Rho, act as the main regulators of the actin cytoskeleton (Campellone and Welch, 2010; Iden and Collard, 2008; Ridley et al., 2003) (Figure
1.3). Rho family proteins are GTPases that are activated by guanine nucleotide exchange factors (GEFs) and inactivated by GTPase activating proteins (GAPs) (Iden and Collard, 2008).
Rho GTPases and their GEFs and GAPs regulate several actin nucleators and actin-nucleation promoting factors (Campellone and Welch, 2010; Iden and Collard, 2008). For instance, Cdc42 and Rac, regulate the activity of Wiskott-Aldrich syndrome protein (WASP)/WASP family verprolin-homology protein (WAVE) proteins respectively, which in turn function to promote
Arp2/3-dependent actin polymerization (Campellone and Welch, 2010). Moreover, different
GTPases, including RhoA, RhoB, RhoC and RhoD, bind and activate several formins
(Campellone and Welch, 2010). Importantly, the expression of several actin assembly factors is misregulated in cancer and correlates with advanced disease (Nurnberg et al., 2011).
13
Figure 1.3 Remodelling of the Actin Cytoskeleton
Extracellular stimuli (1) induce activation of Rho GTPases (2), which activate actin nucleation promoting factors, such as WAVE/WASP proteins (3) that in turn bind and activate the ARP2/3 protein complex (4). Consequently, the Arp2/3 complex binds on the side of an existing actin filament (F-actin) and stimulates the assembly of new actin filaments, which are elongated at the plus (+) end by profilin (5). The force generated during actin polymerization pushes the membrane forward (6). Capping proteins terminate elongation (7). As actin hydrolyzes ATP at the negative (-) end, ADF/cofilin severs and depolymerizes ADP-actin filaments (8). Next, profilin binds monomeric actin and catalyzes the exchange of ADP for ATP (9), thus regenerating the pool of available actin. Formins remain attached to the positive end of actin filaments and promote filament elongation by profilin while preventing capping (10). Figure adapted from (Pollard, 2007).
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Cell motility has been best studied and defined in two-dimensional (2D) surfaces using in vitro assays (Friedl and Wolf, 2009; Ridley et al., 2003). This research has revealed that cell motility is a multi-step and cyclical process that includes 1) generation of cell polarity along the front- rear axis of movement, 2) extension of cell protrusions in the direction of movement, 3) stabilization of protrusions at the leading edge by cell-matrix adhesions, 4) acto-myosin- mediated cell contraction that generates the necessary force for cell movement, and 5) disassembly of cell adhesions rearward of the leading edge and rear-end withdrawal (Friedl and
Wolf, 2009; Ridley et al., 2003) (Figure 1.4). First, a front-rear cell polarization is required for cell motility and involves the organization of the nucleus, the Golgi apparatus, the microtubule
(MT) cytoskeleton (including the centrosome), and cell protrusive activity toward the leading front of movement (Etienne-Manneville, 2008; Iden and Collard, 2008; Ridley et al., 2003).
This allows growth of MTs into the lamella where MT-delivered, Golgi-derived vesicles provide the necessary cellular components for protrusive activity (Ridley et al., 2003). Cdc42 is considered to be a master regulator of polarity in motile cells (Etienne-Manneville, 2008; Iden and Collard, 2008; Ridley et al., 2003) (Figure 1.4). In response to extracellular signals, several downstream pathways, including the Gβγ/p21-activated kinase 1 (PAK1)/PAK-associated GEF
(PIXα) pathway and the phosphoinositide 3-kinase (PI3K) pathway, stimulate the accumulation and activation of Cdc42 in a gradient toward the leading front of migrating cells (Iden and
Collard, 2008; Li et al., 2003; Ridley et al., 2003). Importantly, the Par6/Par3/aPKC polarity complex, which controls AB polarity, also plays a critical role in regulating front-rear polarity in migrating cells (Etienne-Manneville, 2008; Iden and Collard, 2008; Ridley et al., 2003) (Figure
1.4). For instance, activated Cdc42 binds Par6 and promotes activation of aPKC at the leading front (Etienne-Manneville and Hall, 2001), where aPKC phosphorylates and thus inactivates glycogen synthase kinase 3 beta (GSK3β) (Etienne-Manneville and Hall, 2003). This promotes 15
the association of adenomatous polyposis coli (APC) protein with DLG, which capture the MTs at the leading edge and thus allow targeted vesicle delivery to the leading front (Etienne-
Manneville and Hall, 2003). Moreover, the Cdc42/Par6/aPKC complex cooperates with the noncanonical Wnt5a pathway to regulate polarized reorganization of MTs in migratory cells
(Schlessinger et al., 2007). Furthermore, Par3 interacts with the Rac activator T-cell lymphoma invasion and metastasis-1 (TIAM-1) to regulate Rac-dependent actin polymerization at cell protrusions (Iden and Collard, 2008) (Figure 1.4). Next, the assembly of new actin filaments in the leading front of cell protrusions provides the force that pushes the cell membrane forward.
The actin polymerization machinery that drives cell protrusions is regulated primarily by Rac and Rho, which act in negative feedback loops to regulate each other’s activity (Iden and
Collard, 2008; Ridley et al., 2003). Here the Par6 polarity complex also plays a critical role
(Etienne-Manneville, 2008; Iden and Collard, 2008). For example, at the leading front, Par6 recruits the E3 ubiquitin ligase Smurf1, which ubiquitinates and promotes degradation of RhoA at the tips of cell protrusions (Wang et al., 2003) (Figure 1.4). Thus, the Par6-nucleated complexes have a central role in regulating front-rear cell polarity and protrusive activity during cell migration.
Stabilization of newly formed cell protrusions to ECM is necessary for efficient migration
(Friedl and Alexander, 2011; Ridley et al., 2003). Integrins, which are heterodimeric membrane receptors consisting of α and β chains, serve as the main linking proteins for the actin cytoskeleton and ECM (Friedl and Alexander, 2011; Ridley et al., 2003) (Figure 1.4). Upon binding to ECM proteins, such as collagen, fibronectin and laminin, integrins cluster and form focal complexes that are linked to the actin cytoskeleton via several adaptor proteins, including
16
talin, paxillin and vinculin (Friedl and Alexander, 2011; Mitra et al., 2005). In mesenchymal cells, focal complexes rearward of the leading edge evolve into larger and more stable focal adhesions by the concerted action of Rho/Rho kinase (ROCK) signalling and integrin-associated signalling complexes that include the focal adhesion kinase (FAK) and the sarcoma viral oncogene homolog (Src) kinase (Mitra et al., 2005). Focal adhesions are connected to thick bundles of F-actin, known as stress fibers, which undergo acto-myosin-dependent contraction and subsequently strengthen the focal adhesions. Myosin generates contractile force by moving parallel actin filaments relative to one another (Olson and Sahai, 2009). Myosin activity is positively regulated by the phosphorylation of the myosin light-chain (MLC) by a number of kinases, including the Rho kinase (ROCK), the MLC kinase (MLCK), and PAK, and is negatively regulated by the myosin phosphatase (protein phosphatase-1M (PP1M)), which is phosphorylated and inhibited by ROCK (Olson and Sahai, 2009; Ridley et al., 2003). Cell migration proceeds as cells undergo acto-myosin contraction and move over cell adhesions, which serve as traction sites (Ridley et al., 2003). Finally, the cycle of cell migration is completed as focal adhesions in the trailing edge are disassembled by the combined action of extracellular proteases (matrix metalloproteinases (MMPs) and a disintegrin and metalloproteinases (ADAMs)), intracellular proteases (calpain), kinases (including FAK and
Src), and Rho GTPases (Friedl and Alexander, 2011; Mitra et al., 2005; Ridley et al., 2003).
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Front-Rear Axis
Golgi MT Actin-rich Vesicle Cell Protrusion MTOC
Nucleus F-Actin
Focal Stress Adhesion A Fibers Myosin
B
Focal Complex
A Extracellular ECM B Stimuli protein PM PM Receptor Integrins Src Src Paxillin Paxillin Cdc42 TalinFAK TalinFAK P PAR6 Vinculin Vinculin p190 aPKC PAR3 -actininP RhoGEF Smurf TIAM1 Rac1 P RhoA MLC RhoA GSK3 Actin remodelling ROCK MLCK APC P P DLG MLC Actomyosin MLC MLC contraction PP1M MTOC/Golgi orientation ROCK
Figure 1.4 Cell Migration As a Multistep Process
Migratory cells exhibit intrinsic polarity, characterized by the orientation of the nucleus, the Golgi and the microtubule (MT) organizing center (MTOC) along the front-rear axis. MTs provide cellular components, contained within vesicles, at the tip of protrusions. The Cdc42- PAR6 complex regulates cell polarity by controlling both organelle orientation and actin remodelling at cell protrusions (box A). Upon ligand binding, integrin clustering and signalling at the tip of cell protrusions leads to formation of focal contacts, which consist of a number of integrin-associated adaptor proteins and kinases that connect the cell membrane to the actin 18
cytoskeleton and regulate actin dynamics (box B). The focal adhesion kinase (FAK) is a key regulator of focal adhesions. On one hand, phosphorylation of p190RhoGEF by FAK stimulates RhoA activation and thus increases myosin-mediated contraction of stress fibers, which leads to maturation of focal complexes into focal adhesions. On the other hand, phosphorylation of α- actinin by FAK leads to the release of actin stress fibers and disassembly of focal adhesions. Figure adapted from (Iden and Collard, 2008; Mitra et al., 2005; Ridley et al., 2003).
Cell migration in vivo can occur in 2D surfaces, which are found in the walls of blood and lymph vessels and the pleura covering the lungs and thorax wall, or in 3D matrices of connective tissue where several sides of a migrating cell are in contact with other cells or the
ECM (Friedl and Alexander, 2011). Depending on the tumour type and the surrounding environment, cancer cells can adopt different forms of migration: single cell migration, which is enabled by loss of cell-cell adhesions, and collective migration, which occurs when intercellular adhesions are retained (Friedl and Alexander, 2011; Nurnberg et al., 2011). There are two types of single cell migration, mesenchymal and amoeboid, and several forms of collective migration, including clusters and strands (Friedl and Alexander, 2011). In the mesenchymal mode of migration, cells adopt a spindle-shaped morphology, form cell-matrix adhesions that mediate high traction forces, and proteolytically remodel the ECM (Friedl and Alexander, 2011). In the amoeboid mode of migration, cells exhibit a spherical morphology, lack focal adhesions, and do not proteolyse the matrix but instead squeeze through ECM gaps (Friedl and Alexander, 2011).
Collective cell movement requires cell-cell adhesion and coordination between the cells, which move coherently and proteolytically dissolve the ECM (Friedl and Alexander, 2011). Often, the cells at the leading front of cell clusters exhibit a mesenchymal phenotype and generate matrix tracks along which the rest of the cells follow. Alternatively, cancer cells recruit other cell
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types, such as macrophages or fibroblasts, to produce metalloproteases that digest and remodel the matrix and thus promote collective cancer cell migration and invasion (Friedl and
Alexander, 2011). Evidence suggests that cancer cells migrate as single cells toward the blood circulatory system and as clusters of cells toward the lymphatic system (Giampieri et al., 2009).
Importantly, depending on the microenvironmental conditions, tumour cells can switch their migratory phenotype from one form to another (Friedl and Alexander, 2011). The cellular programs underlying this plasticity are currently unclear, although, it is known that TGFβ signalling promotes single cell motility at the invasive front of the primary tumour and in its absence tumour cells move collectively (Giampieri et al., 2009).
Different modes of cell migration are enabled by different types of cell membrane protrusive structures. Cancer cells form several types of protrusive structures, including filopodia, lamellopodia, pseudopodia, invadopodia and membrane blebs (Friedl and Alexander, 2011;
Nurnberg et al., 2011; Olson and Sahai, 2009). Filopodia are thin, finger-like protrusions formed by parallel bundles of actin filaments that are elongated by enabled/vasodilator- stimulated phosphoprotein (Ena/VASP) family of proteins, which prevent capping and branching of F-actin, and are held together by fascin (Mattila and Lappalainen, 2008; Olson and
Sahai, 2009). Filopodia act primarily as sensors for the extracellular environment (Mattila and
Lappalainen, 2008; Olson and Sahai, 2009). Moreover, filopodia enable mesenchymal cell movement and Rac-dependent amoeboid cell movement (Friedl and Alexander, 2011; Mattila and Lappalainen, 2008). Lamellopodia are thin, sheet-like protrusions formed by branched F- actin networks generated by the WAVE/WASP-Arp2/3 actin polymerization machinery (Mattila and Lappalainen, 2008; Olson and Sahai, 2009). Lamellopodia drive mesenchymal cell motility
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on flat 2D substrates (Olson and Sahai, 2009). Pseudopodia are round, lamellopodia-like protrusions of variable size that are formed by a branched network of actin filaments that is remodelled by the WAVE/WASP-Arp2/3 nucleation machinery (Nurnberg et al., 2011; Olson and Sahai, 2009). Pseudopodia facilitate both mesenchymal and amoeboid migration in 3D matrices (Olson and Sahai, 2009). Invadopodia are similar to pseudopodia, except they have
ECM proteolytic activity and their presence correlates with the invasive capacity of tumour cells
(Nurnberg et al., 2011; Olson and Sahai, 2009). Migratory membrane blebs, which are distinct from apoptosis-associated blebs, form by bulging out of the plasma membrane that is devoid of cortical actin (a dense filamentous actin network just under the plasma membrane) (Nurnberg et al., 2011). Blebs are stabilized by newly polymerized cortical actin, in a process that requires formins and ezrin-radixin-moesin (ERM) proteins (Nurnberg et al., 2011; Olson and Sahai,
2009). The actomyosin machinery, regulated by RhoA/ROCK signalling, mediates contraction of cortical actin and thus plays a critical role in bleb-dependent movement (Nurnberg et al.,
2011; Olson and Sahai, 2009). Membrane blebbing enables rapid amoeboid cell migration in
3D environments.
Intensive research in the last few decades has shown that several chemokines (stromal cell- derived factor 1 (SDF-1), CCL5, CCL21), growth factors (HGF, EGF, FGF) and morphogens
(Wnt, TGFβ), released by tumour cells or activated stromal cells, are critical regulators of tumour cell migration (Friedl and Alexander, 2011). These factors engage several downstream signalling networks, including PI3K, Src, and c-Jun N-terminal kinase (JNK) pathways, to regulate Rho GTPase function and actin cytoskeleton dynamics (Friedl and Alexander, 2011).
Currently, we are capable of intersecting these pathways in order to inhibit tumour cell
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migration and invasive capacity. Next, our challenge is to thoroughly understand how the tumour-associated stroma regulates these signalling pathways in cancer cells.
1.1.6. Metastasis – colonization of distant organs
Metastatic tumour formation depends on a series of discrete processes starting with tumour cells invading the adjacent tissue (local invasion), then entering the blood and lymphatic vessels
(intravasation), and being carried away to distant sites where cancer cells escape the circulatory systems (extravasate) and form small nodules (micrometastases) that eventually grow into fully developed macroscopic colonies (known as secondary tumours or metastases) (Hanahan and
Weinberg, 2011; Talmadge and Fidler, 2010) (Figure 1.5). Although metastasis is the main cause of death for cancer patients, the cellular processes and molecular mechanisms that regulate cancer cell intravasation, survival in the circulatory system, extravasation, specificity of metastastic sites and growth in secondary organs remain the least understood aspects of malignancy. During these processes, cancer cells are exposed to different environments and need to respond both physically and biochemically in order to survive (Talmadge and Fidler,
2010; Wirtz et al., 2011). Consistent with this, only a few cells within the primary tumour have the ability to overcome all the challenges encountered during the metastatic process (Talmadge and Fidler, 2010). During intravasation and extravasation, cancer cells squeeze through endothelial cell junctions and thus need to resist severe cell deformations (Wirtz et al., 2011).
This requires increased elasticity of the cytoplasm and the interphase nucleus that is driven by cytoskeletal remodelling, chromatin organization and nuclear envelope interactions, via linkers of the nucleus and cytoskeleton (LINC) proteins, SUN domain-containing proteins and Klarsicht homology (KASH) domain-containing proteins, with the cytoskeleton (Wirtz et al., 2011).
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Once in the circulatory system, cancer cells must overcome shear stress, collisions with other cell types and immunologic surveillance (Talmadge and Fidler, 2010; Wirtz et al., 2011). Shear stress arises from movement of adjacent layers of fluid of different viscosity with different velocities (Wirtz et al., 2011). Activated platelets and leukocytes cluster with cancer cells and protect the latter from shear stress and immunologic surveillance (Gay and Felding-Habermann,
2011; Wirtz et al., 2011) (Figure 1.5). For extravasation to occur, circulating tumour cells have to be either trapped in small vessels, whose diameter is less than that of tumour cells, or adhere to the vessel walls. Adhesion of circulating tumour cells depends on shear flow and is mediated by receptor-ligand interactions between cancer cells and activated endothelium (Gay and
Felding-Habermann, 2011; Wirtz et al., 2011). Activated platelets and leukocytes also facilitate extravasation by mediating tumour cell adhesion to blood vessels, initially via selectins, which are cell adhesion molecules that bind cancer cell-expressed glycoconjugate ligands, including
Cd44 and mucins, and then via integrins, including αIIbβ3 (in platelets), β2 and α4β1 (in leukocytes) and αvβ3 (in cancer cells) (Gay and Felding-Habermann, 2011; Wirtz et al., 2011).
Moreover, it is thought that activated platelets release a multitude of growth factors, including
VEGF, PDGF, TGFβ, and EGF, which act on endothelial cells to induce vascular permeability, thus promoting tumour cell extravasation and invasion into the new microenvironment (Gay and
Felding-Habermann, 2011).
The location of metastatic sites has been a controversial topic in the field of cancer research
(Talmadge and Fidler, 2010). In 1889, Stephen Paget recognized that cancer cells show a specific affinity or tropism for particular organs (Paget, 1989). For instance, breast cancer cells metastasize typically to lungs, bones, liver and less often brain tissue while prostate cancer cells
23
almost exclusively metastasize to bone and liver but not lungs (Paget, 1989; Talmadge and
Fidler, 2010). As a result, Paget first proposed the “seed and soil” hypothesis, which upholds that organ specificity of metastasis corresponds to innate characteristics of the tumour cell, the
“seed”, as well as a particular organ microenvironment, the “soil”, which has to fit the requirements of cancer cells (Paget, 1989). This was later challenged by an alternative hypothesis, which states that the location of a metastatic site depends on the pattern of blood flow (Talmadge and Fidler, 2010). However, both the pattern of blood flow and the local microenvironment may have a complementary role in influencing the site at which secondary metastases grow (Talmadge and Fidler, 2010).
Once at the secondary organ, single tumour cells form micrometastatic lesions that eventually grow into macrometastatic tumours, in a process known as colonization (Talmadge and Fidler,
2010). However, colonization is thought to be a rate-limiting step in the metastatic cascade because many patients have a number of microscopic colonies that do not progress to macrometastases (Bissell and Hines, 2011; Talmadge and Fidler, 2010). It has been suggested that EMT, which is associated with cell cycle arrest in disseminating tumour cells, may prevent efficient growth of metastases (Brabletz, 2012) (Figure 1.5). This was recently supported by the finding that in secondary tissues, cancer cells undergo a mesenchymal-to-epithelial transition
(MET), which facilitates growth of metastases by promoting stem-cell like properties (Ocana et al., 2012), proliferation (Tsai et al., 2012) and alteration of the secretome (Korpal et al., 2011).
Importantly, EMT and MET are regulated by reciprocal interactions between EMT-inducing transcription factors, such as the zinc finger E-box binding homeobox (ZEB) family members and Snail, and MET-inducing microRNAs, including miR-200 and miR-34 families (Brabletz,
24
2012; Thiery et al., 2009). It is currently unknown what signalling molecules induce MET in metastatic cells, however, a TGFβ-related protein, the bone morphogenetic protein (BMP), stimulates expression of miR-200 family members to drive MET during somatic cell reprogramming (Samavarchi-Tehrani et al., 2010). In addition, BMP7 induces MET in renal fibroblasts and in prostate and breast cancer cells in vitro (Brabletz, 2012). So far, the role of
BMP7 in cancer cell metastasis has been investigated by overexpressing the ligand in cancer cells or pre-treating cells with the ligand before injection in mice (Buijs et al., 2012). Thus, in the future it will be important to determine whether BMP specifically induces metastatic colonization in secondary organs.
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Primary Tumour Motility, Invasion and Intravasation
Extravasation Arrest and Adherence Circulation
Platelets & Leukocytes
Activation of Stroma Colonization
MET
Figure 1.5 The Metastatic Cascade
Metastasis is a multistep process that initiates as cancer cells (CCs) acquire a migratory and invasive phenotype through epithelial to mesenchymal transition (labelling is similar to Figure 1.1). Then, CCs detach from the primary tumour, migrate along ECM fibres, invade the local tissue and enter nearby blood/lymphatic vessels (intravasation). In the blood circulatory system, CCs aggregate with platelets and leukocytes, which protect CCs from shear force and immune attack and aid CC adhesion to the vessel walls at distant organs. There, CCs squeeze through the endothelium (extravasate) and migrate into the local tissue. Next, CCs undergo mesenchymal to epithelial transition (MET), which promotes CC proliferation. Moreover, metastatic CCs and the primary tumour CCs secrete signals that modify the microenvironment 26
in the secondary site by remodelling the ECM, activating local fibroblasts, and inducing angiogenesis and inflammation, which support secondary tumour growth (colonization).
1.1.7. The tumour microenvironment
Tumours are considered as aberrant organs composed of cancer cells and multiple other cell types, including fibroblasts, adipocytes, inflammatory cells, and vascular cells, which together with the extracellular matrix (ECM) components, such as proteoglycans, hyaluronic acid and fibrous proteins, constitute the tumour-associated stroma or microenvironment (Bissell and
Hines, 2011; Egeblad et al., 2010) (Figure 1.1). Stromal cells communicate reciprocally with tumour cells and each other via growth factors, cytokines, metabolites and ECM proteins to support tumour initiation, growth and metastasis (Bissell and Hines, 2011; Egeblad et al., 2010).
Evidence suggests that, in specific contexts, the microenvironment restrains and may revert the malignant phenotype in a dominant fashion over the genotype of tumour cells (Bissell and
Hines, 2011). Moreover, tumour malignancy correlates with stage-specific stromal activation, which in later stages is more supportive of tumour progression than in earlier stages (Bissell and
Hines, 2011; Egeblad et al., 2010).
In 1986, Harold Dvorak recognized that “all solid tumours, regardless of their site of origin, require stroma if they are to grow beyond a minimal size of 1 to 2 mm” (Dvorak, 1986).
Moreover, Dvorak proposed that: “tumours behave in the body like wounds and, in fact, induce their stroma by activating the host’s wound healing response” (Dvorak, 1986). During a wound
27
response, tissue injury results in haemorrhage or leakage of plasma, which clots rapidly and forms a gel, consisting of fibrin and fibronectin, that traps platelets and other blood cells
(Dvorak, 1986). Platelets normally take up and sequester a multitude of endogenous angiogenesis-regulatory proteins, such VEGF, FGF2, PDGF and TGFβ, in their alpha granules and secrete these molecules in a wound response (Folkman, 2007). These molecules then can act as mitogens and chemoattractants for connective tissue cells, including fibroblasts, inflammatory cells and endothelial cells that communicate in concert with each other to rebuild the damaged tissue. Dvorak hypothesized that similarly to a wound response, tumour-associated stroma becomes “reactive” upon leakage of plasma proteins from hyperpermeable blood vessels that initiate a cascade of events that result in replication and migration of inflammatory cells and fibroblasts and the formation of new blood vessels (Dvorak, 1986). Moreover, he realized that differently from wound healing, fibroblast proliferation and inflammation is persistent in the tumour-associated stroma and thus tumours can be considered as wounds that do not heal
(Dvorak, 1986).
In the last 25 years, research has shown that indeed cancer cells co-opt and manipulate the normal wound healing response in order to drive tumour growth both in the primary and secondary sites (Bissell and Hines, 2011; Folkman, 2007; Mantovani et al., 2008). As mentioned above, tumour cells secrete factors that stimulate recruitment of endothelial cells or bone marrow derived cells, which form new blood vessels (Folkman, 2007; Lyden et al., 2001), and inflammatory cells, such as macrophages and myeloid progenitors, which support tumour cell proliferation, evasion of apoptosis, angiogenesis and metastasis (Egeblad et al., 2010;
Mantovani et al., 2008) (Figure 1.2). Other stromal components are also involved in tumour
28
growth and metastasis (Figure 1.2). For example, mesenchymal stem cells (MSCs) interact directly with cancer cells by secreting Ccl5, a chemokine that binds its cognate receptor in cancer cells and promotes their invasive behaviour (Karnoub et al., 2007). Lymphatic endothelial cells produce cytokines, such as Ccl21, that guide tumour cells toward the lymphatic system (Tammela and Alitalo, 2010). Adipocytes are also emerging as important components of the tumour-associated stroma as they secrete collagen VI, adiponectin and IL-6 that promote tumour cells survival, growth and invasive capacity (Dirat et al., 2011; Iyengar et al., 2005;
Landskroner-Eiger et al., 2009).
The process of metastatic colonization is also tightly linked to the function of the microenvironment (Egeblad et al., 2010; Talmadge and Fidler, 2010). Accumulating evidence suggests that primary tumour cells prepare the microenvironment that they will eventually colonize (also known as the premetastatic microenvironment or niche), in order to support metastatic cell survival and growth by inducing angiogenesis, endothelial permeability and remodelling of ECM in the premetastatic niche (Egeblad et al., 2010; Gao et al., 2008; Kaplan et al., 2005; Peinado et al., 2012; Psaila and Lyden, 2009). Both signalling molecules (VEGF and lysyl oxidase) and microvesicles (including exosomes) secreted by cancer cells have been shown to mediate the communication with the premetastatic niche (Egeblad et al., 2010; Kaplan et al., 2005; Peinado et al., 2012; Psaila and Lyden, 2009). Considering the complexity of the cross talk between tumour and stromal cells, it is imperative that these interactions are fully understood in order to better target tumours in patients.
29
1.1.8. Fibroblasts as components of the tumour microenvironment
Fibroblasts constitute, in many cases of carcinoma, the most abundant cell population of the tumour-associated stroma (Kalluri and Zeisberg, 2006). Fibroblasts are highly heterogeneous cells, which are broadly defined as non-vascular, non-epithelial and non-inflammatory cells that are the primary components of the connective tissue (Kalluri and Zeisberg, 2006; Rasanen and
Vaheri, 2010). Fibroblasts are embedded within the matrix of the connective tissue and regulate
ECM turnover by synthesizing ECM components, including type I, III and V collagens, fibronectin, and MMPs (Egeblad et al., 2010; Kalluri and Zeisberg, 2006). Fibroblasts also secrete type IV collagen and laminins, which constitute the basement membrane that plays a critical role in the maintenance of epithelial AB polarity. Moreover, fibroblasts secrete growth factors that help maintain epithelial homeostasis (Egeblad et al., 2010; Kalluri and Zeisberg,
2006). Fibroblasts also function in wound repair by invading lesions and producing ECM that functions as scaffold for other cells and facilitates contractions of healing wounds (Egeblad et al., 2010; Kalluri and Zeisberg, 2006; Rasanen and Vaheri, 2010). Fibroblasts from wounds or scar tissue exhibit an activated phenotype, characterized by enhanced secretion of ECM proteins
(including type I collagen and tenascin C), ECM-degrading proteases (including MMP2, MMP3 and MMP9) and growth factors (including HGF, IGF, NGF, Wnt1, EGF and FGF2), and they have a higher proliferation rate than their normal counterparts (Kalluri and Zeisberg, 2006;
Rasanen and Vaheri, 2010). Similarly, fibroblasts in close proximity to cancer cells are also activated and are defined as cancer associated fibroblasts (CAFs). In wound healing, fibrosis and cancer, TGFβ (secreted by injured epithelial cells or cancer cells), intercellular-adhesion molecule 1 (ICAM1) and vascular-cell adhesion molecule 1 (VCAM1) (secreted by leukocytes), reactive oxygen species and complement factor C1 have been found to signal the transition of normal fibroblasts to their active phenotype (Bissell and Hines, 2011; Kalluri and Zeisberg, 30
2006). In contrast to wound healing, however, fibroblasts in fibrotic tissue and cancer are perpetually activated and the signals responsible for this effect are currently unknown.
Cancer-associated fibroblasts can be divided into at least two distinct subtypes 1) reprogrammed variants of connective tissue-derived fibroblasts and 2) myofibroblasts, which express α-smooth muscle actin (SMA) (Bissell and Hines, 2011; Egeblad et al., 2010). Myofibroblasts are rarely found in healthy epithelial tissue and their presence is more common in wounds and fibrotic tissue (Bissell and Hines, 2011; Egeblad et al., 2010; Kalluri and Zeisberg, 2006). The origins of CAFs is currently unclear, however, evidence suggests that they originate from local residing fibroblasts, from adipocytes, from pericytes, from bone marrow derived mesenchymal cells, or by epithelial- or endothelial- to mesenchymal transitions (Egeblad et al., 2010; Rasanen and
Vaheri, 2010; Thiery et al., 2009). So far, CAFs have been studied as a singular cell population and thus the contributions of each subtype of cells to cancer remain to be resolved. Several
CAF-expressed-markers, including PDGFRβ, carbonic anhydrase IX (CAIX), and α-SMA correlate with tumour recurrence, metastasis and/or poor prognosis (Rasanen and Vaheri, 2010).
CAFs are intimately involved in the initiation and progression of cancer (Kalluri and Zeisberg,
2006; Rasanen and Vaheri, 2010). They secrete several factors, including HGF and SDF-1, to promote epithelial cell neoplastic transformation and cancer cell proliferation (Bhowmick et al.,
2004; Orimo et al., 2005). In addition, CAFs interact with other stromal components via paracrine loops to stimulate tumour-enhancing inflammation, angiogenesis and lymphangiogenesis (Erez et al., 2010; Kalluri and Zeisberg, 2006; Orimo et al., 2005; Tammela and Alitalo, 2010). Also, both protease- and mechanotransduction force-dependent ECM remodelling by CAFs, is essential for tumour cell invasion and metastasis (Gaggioli et al., 2007;
31
Goetz et al., 2011; Kalluri and Zeisberg, 2006; Sternlicht et al., 1999). Although CAFs are predominant constituents of the tumour microenvironment and are key determinants of malignant progression, the paracrine signals that mediate direct cross talk between CAFs and tumour cells in metastasis are poorly understood.
1.1.9. Identification and function of cancer stem-like cells
In the last two decades, it has been shown that a subclass of cells within liquid (Lapidot et al.,
1994) or solid tumours (Al-Hajj et al., 2003), termed cancer stem-like cells (CSCs), have self- renewing capacity and even express markers and share transcriptional profiles with normal stem cells in the tissue of origin (Hanahan and Weinberg, 2011). Accordingly, CSCs are able to efficiently give rise to new tumours upon inoculation into recipient host mice (Hanahan and
Weinberg, 2011; Visvader, 2011). The origins of CSCs remain unclear and might be different from one tumour type to another. CSCs may rise from oncogenically transformed normal stem cells or from their partially differentiated progenitor cells, as observed for instance in intestinal and prostate cancer (Visvader, 2011). Alternatively, CSCs may rise from differentiated cells that acquire self-renewal capabilities, possibly through the involvement of EMT (Mani et al.,
2008; Morel et al., 2008), although the newly-discovered EMT activator, the paired-related homeobox transcription factor 1 (Prrx1), suppresses stemness traits (Ocana et al., 2012). This field of research is still in its early stages and a lot of questions remain with regards to the stem cell-like properties of CSCs and their importance in tumourigenesis (Clevers, 2011).
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1.2. Noncanonical Wnt-Planar Cell Polarity Pathway
1.2.1. Planar cell polarity and its manifestations
Planar cell polarity (PCP), also known as tissue polarity, refers to organization of cell behaviour at the tissue level in a plane perpendicular to the axis of apical-basal cell polarity (Bayly and
Axelrod, 2011; Gray et al., 2011; Wallingford, 2012; Wu and Mlodzik, 2009). PCP requires the establishment of asymmetrical organization of protein complexes or subcellular structures within cells or asymmetric orientation of a group of cells with the alignment of these asymmetries across a tissue (Gray et al., 2011; Wu and Mlodzik, 2009). Moreover, PCP is coordinated at the tissue level with regards to the anteroposterior (AP), dorsoventral (DV) and left-right (LR) body axes (Gray et al., 2011).
Planar cell polarity (PCP) was first studied in the fruit fly, Drosophila melanogaster, where PCP is manifested in the AP orientation of hair bristles in the thorax and abdomen, the DV arrangement of ommatidia in the compound eye, the proximal-distal (PD) organization of leg cells and leg segments and the PD orientation of wing hairs from hexagonal epithelial cells
(Bayly and Axelrod, 2011; Wu and Mlodzik, 2009; Zallen, 2007) (Figure 1.6 A-B). Here, PCP directs polarity by employing a range of cellular mechanisms in different tissues under different biological contexts. For instance, in the fly wing, every epithelial cell reorganizes its actin cytoskeleton to generate a distally pointed actin-based hair (cytochrome) at its distal vertex
(Bayly and Axelrod, 2011; Wu and Mlodzik, 2009; Zallen, 2007) (Figure 1.6A). In the compound eye of Drosophila, a group of cells that form a unit eye, termed ommatidia, make a coordinated decision, which requires transcriptional activation and intercellular communication
(Zallen, 2007). In the ommatidia, the R3 and R4 photoreceptor cells differentiate in an 33
asymmetric fashion and the entire structure rotates as a unit in opposite directions in the dorsal and ventral halves of the eye (Bayly and Axelrod, 2011; Wu and Mlodzik, 2009; Zallen, 2007)
(Figure 1.6B). PCP can also influence the orientation of bristles, which consist of a four-cell cluster including a shaft, socket, sheath and neuron that arise from a single sensory organ precursor cell (Shulman et al., 1998; Zallen, 2007). Asymmetric and oriented division of the latter into its daughter cells is regulated by PCP signalling, thus indicating that the polarity of the precursor cell influences the organization of its descendants (Shulman et al., 1998; Zallen,
2007). PCP also regulates the morphogenesis of the fly dorsal thorax epithelium by regulating cell junction tension, which defines the pattern of local tissue contraction and shape of the epithelium mainly via oriented cell rearrangements (Bosveld et al., 2012). Thus, regulation of the actin cytoskeleton, oriented cell division and group-cell rotation are some of the cellular mechanisms by which PCP signalling regulates tissue polarity in the fly (Zallen, 2007).
Similarly, in vertebrates, PCP directs polarity in a multitude of different tissues and in different biological contexts (Figure 1.6). Some examples include, convergent and extension (CE) movements during gastrulation and neurulation, the orientation of hair bundles in inner ear sensory cells, the orientation of body hair, directional beating and assembly of cilia and migration of facial branchiomotor neurons (Gray et al., 2011; Wallingford, 2012). During gastrulation, CE movements of dorsal mesodermal cells allow the extension of the embryonic tissue along the AP axis and narrowing of the embryo along the mediolateral (ML) axis (Gray et al., 2011; Wallingford, 2012) (Figure 1.6C). At first, cells align, elongate and extend protrusions in the ML direction. Then, they form stable cell-cell contacts (intercalations) between anterior and posterior neighbouring cells within a plane (mediolateral intercalations)
34
and in the more shallow and deeper cell layers (radial intercalations), which allow the coordinated and enhanced movement of the cells toward the dorsal midline (Gray et al., 2011;
Wallingford, 2012). Similarly, during neurulation, CE movements of neuro-ectodermal cells allow the fusion of the neural folds to form the neural tube (Gray et al., 2011; Wang et al.,
2006). During both gastrulation and neurulation, PCP signalling regulates and coordinates polarized cell behaviour, such as cell polarity, protrusive activity, directional migration as well as oriented cell division (Gong et al., 2004; Gray et al., 2011). In addition, PCP signalling in vertebrates is essential for establishing left-right embryonic asymmetry by orienting the cilia in the AP direction and thus regulating the leftward cilia-driven fluid flow, which is required for left-right asymmetric gene expression in the mouse ventral node, zebrafish Kupffer’s vesicle and Xenopus gastrocoel roof plate (Antic et al., 2010; Borovina et al., 2010; Gray et al., 2011).
Here, the cells display planar polarization of the cilia, which protrude from near posterior portion of each cells’ apical surface and are tilted in the posterior direction in a PCP pathway- dependent manner (Gray et al., 2011). Moreover, in mice, PCP signalling controls the ML alignment of the kinocilium (microtubule-based cellular protrusion) and the adjacent stereocilia
(actin-based cellular protrusions), which make up the sensory hair bundles in the inner ear cells
(Gray et al., 2011; Wang et al., 2006) (Figure 1.6D). PCP signalling is also critical for the global AP alignment of body hair by regulating cell shape changes, cytoskeletal polarization and polarized gene expression in nascent hair follicles (Devenport and Fuchs, 2008; Gray et al.,
2011; Guo et al., 2004). Disruption of PCP signalling results in dysmorphogenesis of a wildly diverse array of tissues (Wallingford, 2012). As a result, aberrant PCP signalling leads to deafness, heart defects, polycystic kidney disease, ciliopathy and craniorachischisis (an open neural tube) (Gray et al., 2011; Simons and Mlodzik, 2008; Wu et al., 2011; Yang, 2012).
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1.2.2. Molecular PCP components in the fly
The molecular components involved in establishing PCP were first discovered in Drosophila genetic screens that used the ommatidia, sensory bristles or wing hairs as model systems (Bayly and Axelrod, 2011; Lawrence et al., 2007; Wu and Mlodzik, 2009; Zallen, 2007). These studies allowed the discovery of a number of genes involved in PCP that were divided in two distinct groups, or modules, the core Frizzled/PCP module and the Fat/Dachsous module, according to the morphological manifestations observed upon their mutation or misexpression in the fly tissue (Bayly and Axelrod, 2011; Lawrence et al., 2007; Wu and Mlodzik, 2009; Zallen, 2007).
The core Frizzled/PCP module, consists of a seven-pass transmembrane protein, Frizzled (Fz,
Fzd in vertebrates); a four-pass transmembrane protein, van Gogh/Strabismus (Vang/Stbm, van
Gogh-like (Vangl) in vertebrates); a seven-pass transmembrane atypical catherin,
Flamingo/Starry Night (Fmi/Stan, the cadherin EGF LAG seven-pass G-type receptor (Celsr) in vertebrates) and the cytoplasmic proteins: Dishevelled (Dsh, Dvl in vertebrates), Prickle (Pk) and Diego (Dgo, Diversin/Inversin (Div/Inv) in vertebrates/mouse respectively) (Bayly and
Axelrod, 2011; Wu and Mlodzik, 2009; Zallen, 2007). Importantly, mutations of Dsh, Pk, Fmi or Dgo result in PCP defects within the mutant cells, indicating that these factors are only involved in conducting PCP signalling in a cell autonomous manner (Wu and Mlodzik, 2009).
In contrast, mutations of Fz and Vang, in addition to PCP defects within mutant cells, result in reversal of the polarity of adjacent, wild type cells, indicating that these factors act both in a cell autonomous and non-autonomous manner to coordinate and propagate polarity at a more global level (Lawrence et al., 2007; Wu and Mlodzik, 2009; Zallen, 2007). The expression of Fmi, which does not have a non-autonomous effect on cellular polarity, is required for the non- autonomous effects of Fz (Wu and Mlodzik, 2009). The second set of PCP genes, includes Fat
(Ft, Fat in vertebrates) and Dachsous (Ds, Dchs in vertebrates), two large atypical catherins that 36
can interact heterophilically across cell boundaries, and the transmembrane, Golgi protein, Four- jointed (Fj, Fjx in vertebrates), a kinase that acts in a graded fashion to modulate Ft/Ds activity
(Bayly and Axelrod, 2011; Blair, 2012; Goodrich and Strutt, 2011). Interference with normal
Ft, Ds and Fj expression results in randomization of PCP within mutant cells and reversal of the polarity of the neighbouring cells, indicating that these genes act in both autonomous and non- autonomous manners to regulate PCP (Lawrence et al., 2007; Zallen, 2007). Moreover, mutations in the Ft/Ds group alter the shape of the wings and legs and disturb tissue growth through regulation of the Hippo pathway (Lawrence et al., 2007; Sopko and McNeill, 2009). In addition to the two main PCP modules that include genes with a predominant PCP function, several genes, such as Rho GTPases, ROCK, aPKC and Scribble, have been identified that are required for polarization only in specific tissues and are referred to as “the effector genes”
(Bayly and Axelrod, 2011; Wu and Mlodzik, 2009). Moreover, recent genetic analyses in the fly have revealed novel regulators of PCP whose function has yet to be studied in detail (Weber et al., 2012).
1.2.3. Models of PCP signalling in the fly
Although great progress has been made in identifying the fly PCP factors, it is still unclear how planar cell polarity signalling is initiated, conducted within the polarized cells and propagated across the tissue (Bayly and Axelrod, 2011; Blair, 2012; Lawrence et al., 2007; Wu and
Mlodzik, 2009). Indeed, the initial signal that biases the asymmetrical subcellular localization of core Fz/PCP molecules and directs planar polarity at the tissue level remains unknown. Fz and Vang double mutant clones display phenotypes similar to single Fz mutant clones, suggesting that PCP signalling is instructed by Fz activity (Wu and Mlodzik, 2009). Moreover,
37
non-autonomous Fz signalling is required before core PCP molecules become asymmetrically localized, suggesting that Fz non-autonomous signalling has an instructive role in the global polarization of tissues (Wu and Mlodzik, 2009). Fz is the receptor of the Wnt morphogen, which could signal PCP from a distant source and thus instruct graded Fz activity. However, in the fly, there is no direct evidence that Wnt ligands act to trigger PCP. Genetic studies suggest that the fly Wnt4 (dWnt4) ligand can alter PCP in the eye and wing but this may be due to indirect effects on the expression and function of other genes (Wu and Mlodzik, 2009). The
Ft/Ds module was initially proposed to act upstream of the Fz/PCP core module to regulate tissue polarity in a global manner. However, the current consensus is that the Ft/Ds pathway acts in parallel to the Fz/PCP pathway and may influence core protein polarity only in particular contexts and tissues (Bayly and Axelrod, 2011; Blair, 2012; Gray et al., 2011; Lawrence et al.,
2007). As a result, the search continues for the mystery factor X that first signals PCP in the fly.
The molecular mechanisms employed by the core Fz/PCP module in conducting tissue polarity are better understood. Fz/PCP signalling is mediated by complex interactions between the core components that function in regulatory loops rather than a linear pathway (Wu and Mlodzik,
2009). This is accompanied by an underlying asymmetric distribution of core PCP proteins along the PCP axis, which is necessary for PCP signalling (Bayly and Axelrod, 2011; Wu and
Mlodzik, 2009) (Figure 1.6). For instance, in the fly wing cells, Vangl and Pk are enriched at the proximal and Fz, Dsh, and Dgo at the distal apical cell surface (Wu and Mlodzik, 2009).
Before PCP is established, the core PCP components are localized uniformly around the apical- lateral cell cortex in epithelial cells (Wu and Mlodzik, 2009). Frizzled recruitment and activity at the cell surface initiates apical recruitment of other core PCP components that interact with
38
each other to maintain their apical membrane association in a positive feedback loop (Wu and
Mlodzik, 2009). Polarization of the core components along the apical-basal axis is a prerequisite for their subsequent asymmetrical localization along the PCP axis (Wu and
Mlodzik, 2009). Once at the apical surface, Fmi-Fz complexes are endocytosed and transported distally in vesicles on microtubules aligned along the proximal-distal axis parallel to the cell surface (Shimada et al., 2006). Then, Fz, which is enriched at the distal cell surface, binds and retains Vang on the proximal surface of the neighbouring cell (Wu and Mlodzik, 2009).
Moreover, Pk antagonizes Fz-Dsh interaction while Dgo interacts with Pk and Vang and may counteract Pk activity in order to allow the Fz-Dsh complexes to form at the distal surface (Wu and Mlodzik, 2009). Fmi localizes to both proximal and distal surfaces, interacts homophilically in trans between neighbouring cells and is thought to stabilize the Fz/Dsh/Dgo and Vang/Pk complexes through interaction with Fz and Vang (Wu and Mlodzik, 2009). Once segregated in opposite sides of the cell, the Fz-Dsh-Dgo complex acts positively to promote
PCP signalling through activation of Dsh and its effectors, while the Vang-Pk complex functions to limit Dsh activation by feedback loop interactions (Wu and Mlodzik, 2009). Thus, heterophilic core protein interactions at cell boundaries result in subcellular asymmetry that is critical for conducting the PCP signal across the tissue.
1.2.4. PCP signalling in vertebrates
The core Fz/PCP genes are evolutionary conserved and required for PCP establishment in vertebrates (Gray et al., 2011; Wallingford, 2012; Wu and Mlodzik, 2009). The number of vertebrate core PCP homologs is considerably higher than in the fly, including ten Frizzled
(Fzd1-10), three Dvl (Dvl1-3), two Vangl (Vangl1-2), two Pk (Pk1-2) and three Celsr (Celsr1-3)
39
genes. Even though functional redundancy between the different homologs is common, single and compound mutants of several core PCP genes manifest PCP defects in vertebrates (Gray et al., 2011). Moreover, the phenomenon of Fzd and Vangl nonautonomy observed in the fly also occurs in vertebrates. For instance, morphological and molecular polarization of hair follicles in the mouse epidermis require non-autonomous functions of Vangl2 (Devenport and Fuchs,
2008). In addition, asymmetric localization of the core PCP molecules is conserved in vertebrates (Wallingford, 2012) (Figure 1.6 C-E). For instance, in the mouse node, overexpressed Pk2 and Vangl1 localize to anterior cell edges (Antic et al., 2010), while overexpressed Dvl localizes to the posterior cell edges (Hashimoto et al., 2010). Asymmetric distribution of core PCP proteins is also observed in dynamically remodelled tissue, where Pk accumulates in puncta in mesodermal and neuroectodermal cells (Ciruna et al., 2006; Narimatsu et al., 2009; Yin et al., 2008) (Figure 1.6C). The polarized subcellular localization of core PCP molecules in vertebrates suggests that the PCP signalling mechanisms are at least at some extent evolutionary conserved (Gray et al., 2011; Wu and Mlodzik, 2009). Indeed, Vangl2 and Celsr1 are dependent on one another for their proper asymmetric distribution along the AP axis in the developing epidermis (Devenport and Fuchs, 2008). Moreover, Fzd6 association with the membrane dependents on both Celsr and Vangl2 (Devenport and Fuchs, 2008). Furthermore, membrane association and asymmetric localization of Dvl and Pk depends on Fzd and Vangl expression (Ciruna et al., 2006; Takeuchi et al., 2003; Veeman et al., 2003; Yin et al., 2008).
Similar to the fly system, Pk inhibition of Frizzled-mediated membrane association of Dvl is also conserved in vertebrates (Carreira-Barbosa et al., 2003; Jiang et al., 2005). However, the core PCP molecules are not always asymmetrically distributed with the same partners as observed in the fly (Gray et al., 2011; Wallingford, 2012). For instance, in inner ear cells, Dvl accumulates at the lateral cell edges Wang, 2005 #433}, whereas Fzd3/6 accumulates with
40
Vangl2 and Pk along the medial cells edges (Montcouquiol et al., 2006; Narimatsu et al., 2009;
Wang et al., 2006) (Figure 1.6D). These findings suggest that in vertebrates other mechanisms are implicated in establishing PCP. Consistent with this, genetic studies indicate that a number of novel proteins regulate vertebrate PCP by employing several different molecular mechanisms
(Bayly and Axelrod, 2011; Gray et al., 2011; Wallingford, 2012). For instance, the receptor tyrosine kinase Ror2 binds Wnt5a and regulates PCP in the developing limb bud by inducing
Vangl2 phosphorylation and enhancing Vangl2 asymmetric localization in chondrocytes (Gao et al., 2011). The receptor-like tyrosine kinase (Ryk), a Wnt binding protein, regulates PCP by interacting with Vangl2 and promoting its stability (Andre et al., 2012). Vertebrate protein tyrosine kinase 7 (PTK7) regulates vertebrate CE movements (Yen et al., 2009) by recruiting
Dvl to the plasma membrane through Fzd (Shnitsar and Borchers, 2008) and receptor of activated protein kinase C 1 (RACK1) (Wehner et al., 2011). In addition, Smurf ubiquitin ligases control PCP and CE in mice by physically interacting with Dvl that is bound to Par6 and targeting Pk1 for ubiquitin-mediated degradation (Narimatsu et al., 2009). Moreover, XGAP, a
GTPase-activating protein for ADP ribosylation factors (ArfGAP), interacts with the
Par6/aPKC/14-3-3ε polarity complex to direct its localization to mediolateral ends of dorsal mesoderm cells and restrict their protrusive activity in CE movements in Xenopus (Hyodo-
Miura et al., 2006). The number of genes involved in vertebrate PCP signalling is rapidly increasing and future studies will be necessary to understand their function in different biological contexts (Wallingford, 2012).
41
A Wing hairs B Ommatidia P D D
Equator
5 Actin- R4 6 V based 8 7 hair R3 2 1
C D E Ependymal Convergent extension Cochlear hair cells multiciliated cells C R A M L L M L kinocilium
stereocilium
P cilia
basal bodies
Figure 1.6 PCP in Drosophila and Vertebrates
(A) The fly wing epithelium is polarized in the proximal (P) to distal (D) axis. Each cell extends an actin-based protrusion (hair) in the distal vertex (top panel). Fzd (dark green) and Dvl (light green) localize at the distal apical membrane while Vangl (orange) and Pk (yellow) localize at the proximal apical membrane (bottom panel). (B) In the developing fly eye, the ommatidia, which consist of a cluster of cells (including R3 and R4 photoreceptor cells), are organized along the equator (top panel). Fzd localizes to the R3 side of the R3/R4 membrane border while Vangl localizes to the R4 cell membrane (bottom panel). (C) During CE movements in vertebrates, cells extend protrusions in their medial (M) and lateral (L) ends, intercalate and move towards the medial axis thus redistributing along the anterior (A) to posterior (P) axis (top panel). Dvl and Pk puncta localize posteriorly and anteriorly respectively
42
(bottom panel). (D) In the mouse cochlea, hair cells are polarized along the ML axis, as revealed by the orientation of stereocilia (actin-based protrusions) and kinocilium (tubulin-based protrusion) (top panel). Dvl localizes laterally while Vangl, Pk and Fzd localize along the medial membrane (bottom panel). (E) In the mouse brain, ependymal cells are polarized along the caudal (C) to rostral (R) axis as revealed by the orientation of basal bodies and cilia (top panel). The asymmetrical distribution of Vangl is shown (bottom panel). Figure was adapted from (Goodrich and Strutt, 2011; Wallingford, 2012).
Unlike in the fly system, genetic studies in different vertebrate model systems have revealed that
Wnt morphogens play an important role in providing global regulation of tissue polarity
(Wallingford, 2012) and might even trigger the initial asymmetry that is propagated across the tissue (Goldstein et al., 2006; Gros et al., 2009). For instance, in zebrafish, silberblick (an orthologue of human Wnt11) (Heisenberg et al., 2000) and pipetail (an orthologue of human
Wnt5b) (Kilian et al., 2003) are specifically required for CE movements. Similarly, in Xenopus laevis, overexpressed Wnt11 (Tada and Smith, 2000) and Wnt5a (Moon et al., 1993;
Wallingford et al., 2001b) interfere with CE movements. Moreover, in mice, Wnt ligands regulate PCP in CE movements (Qian et al., 2007), primitive muscle fibre orientation (Gros et al., 2009), kidney tubule morphogenesis (Karner et al., 2009) and cartilage extension in mouse limb buds (Gao et al., 2011). Importantly, knypek, a heparan sulphate proteoglycan, potentiates
Wnt11 signalling and promotes polarized cell behaviours during gastrulation movements in zebrafish (Topczewski et al., 2001). Even though it is clear that Wnts are critical in regulating
PCP in vertebrates, the molecular mechanisms involved are poorly understood.
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1.2.5. Wnt structure and post-translational modifications
Wnts belong to a family of secreted signalling molecules (19 members in mammals) that regulate a myriad of cell biological processes, including cell proliferation, differentiation, survival, polarity, migration and stem-cell self-renewal, during embryonic development, tissue homeostasis and disease (Willert and Nusse, 2012). The name “Wnt” was derived from the
Drosophila Wnt homologue, wingless (wg), and mouse Int1, an oncogene often activated upon insertional mutagenesis by the mouse mammary tumour virus (MMTV) in mammary carcinoma
(Rijsewijk et al., 1987). All Wnt proteins are characterized by the presence of 22 or 24 cysteine residues, most of which are thought to form intramolecular disulphide bonds that are critical for
Wnt structure and function (Willert and Nusse, 2012). More than thirty years after the discovery of Wnts, the crystal structure of Xenopus Wnt8 (XWnt8) in complex with the cysteine-rich domain (CRD) of mouse Frizzled8 was recently resolved (Janda et al., 2012). This crystal indicated that XWnt8 has a two-domain structure, analogous to a “hand” with “thumb” and “index finger” grabbing the Fzd8 CRD (Janda et al., 2012). The “thumb” contains the amino-terminal domain (NTD), comprised of seven alpha helices held together by five disulphide bonds, while the “index finger” contains the carboxy-terminal domain (CTD), composed of two beta sheets held together by six disulphide bonds (Janda et al., 2012). The contact point between the XWnt8 NTD (thumb) and the Fzd8-CRD is mediated by a palmitoleic acid lipid group that protrudes from serine 187 (a conserved site required for Wnt palmitoylation and function (Takada et al., 2006)) into a deep groove in the CRD of the receptor (Janda et al.,
2012). The contact point between the CTD of XWnt8 and receptor CRD is mediated by hydrophobic amino acids, which are also conserved among different Wnts (Janda et al., 2012).
44
Wnts are subject to posttranslational modifications, including glycosylation and palmitoylation, which drive their tight association with the plasma membrane and ECM and are required for
Wnt activity (Coudreuse and Korswagen, 2007; Port and Basler, 2010; Willert and Nusse,
2012). In particular, Wnts are palmitoylated in a manner that is dependent on Porcupine, a multi-transmembrane protein that resides in the endoplasmic reticulum (ER) and is essential for
Wnt secretion and function (Herr and Basler, 2012; Kadowaki et al., 1996; Takada et al., 2006).
In addition, some Wnt ligands, for instance Wnt5a and Wnt11, can also be sulfonated by tyrosyl protein sulfotransferase-1 (TPST-1) and this modification enhances their signalling activity (Cha et al., 2009). Moreover, glycophosphatidyinositol (gpi)-like anchors can also be added to Wnts, for instance Wnt1 and Wnt3a, in a manner that is dependent on the ER-resident glycoprotein
Oto, which regulates retention of Wnts in the ER and Wnt signalling (Zoltewicz et al., 2009).
From the ER, Wnt transport to the Golgi is facilitated by two p24 protein family members,
Éclair and Emp24, which are involved in cargo selection from the ER to Golgi (Port et al.,
2011), and from there to the plasma membrane by the seven-pass transmembrane protein
Wntless (Wls), whose function is essential for Wnt secretion (Banziger et al., 2006; Bartscherer et al., 2006; Goodman et al., 2006; Herr and Basler, 2012). Once at the plasma membrane,
Wnts, which are highly hydrophobic, depend on several factors to function as long range signalling molecules. In the fly, heparan sulphate proteoglycans (HSPGs) of the glypican family regulate Wg gradient formation and signalling by a restricted diffusion mechanism (Baeg et al., 2001; Han et al., 2005). In addition, high-density lipoproteins particles, which consist of a central core of triglycerides and cholesterol enveloped by an outer phospholipid monolayer that is scaffolded by apoliproteins, act to solubilize Wg and are required for long-range Wg signalling (Panakova et al., 2005). Recently, Secreted Wg-interacting molecule (Swim), a putative member of the Lipocalin family of extracellular transport proteins, has also been shown
45
to carry Wg and promote its long-range signalling (Mulligan et al., 2012). Finally, exosome- like vesicles secreted at the Drosophila neuromuscular junction carry Wg in association with
Wntless (Korkut et al., 2009) and mammalian Wnts are secreted on exosomes (Beckett et al.,
2012; Gross et al., 2012; Ratajczak et al., 2006). However, more investigation is required to establish the significance of these mechanisms in different Wnt-dependent processes.
1.2.6. Wnt signalling pathways
Wnts trigger several signalling cascades that are broadly categorized as canonical (Wnt-β- catenin pathway) and noncanonical pathways (including the Wnt-PCP pathway) (Angers and
Moon, 2009; Gao and Chen, 2010; Willert and Nusse, 2012) (Figure 1.7). Importantly, the signalling pathways activated by Wnts depend on the expressed repertory of receptors and downstream effectors within a particular cell type rather than Wnt intrinsic properties (Anastas and Moon, 2013; Willert and Nusse, 2012). For instance, both Wnt5a and Wnt11, which regulate a number of PCP processes, can also activate canonical signalling (Willert and Nusse,
2012). The Wnt-β-catenin signalling pathway ultimately leads to the regulation of a β-catenin- dependent transcriptional program (Angers and Moon, 2009) (Figure 1.7A). In the absence of
Wnt stimulation, cytoplasmic β-catenin is recruited into a “destruction complex”, consisting of adenomatous polyposis coli (APC) and Axin, which stimulate phosphorylation of β-catenin by glycogen synthase kinase 3 beta (GSK3β) and casein kinase 1 (Ck1). This leads to ubiquitylation and proteasomal degradation of β-catenin. The binding of Wnts to Frizzled, which act as G protein coupled receptors (GPCRs) (Angers and Moon, 2009), and lipoprotein receptor-related proteins 5 (LRP5) or LRP6 coreceptors leads to Dvl activation, which polymerizes and promotes clustering of Wnt-Fzd-LRP5/6 complexes (Gao and Chen, 2010). 46
This leads to phosphorylation of LRP5/6 by GSK3β and Ck1 and recruitment of Axin to the plasma membrane. Consequently, β-catenin is released from the destruction complex and translocates to the nucleus where it acts as a co-activator for the T-cell factor (TCF) family of transcription factors and activates transcription of Wnt target genes (Angers and Moon, 2009).
The noncanonical Wnt pathways, include at least two pathways, the Wnt-PCP and the Wnt-Ca+2 pathways, which are not only independent of β-catenin function but also antagonize Wnt-β- catenin signalling (Angers and Moon, 2009). In vertebrates, accumulating evidence shows that the Wnt-PCP pathway regulates the stability of core PCP proteins and their asymmetric distribution (Andre et al., 2012; Gao et al., 2011; Narimatsu et al., 2009). For instance, upon
Wnt binding to Frizzled receptors, Dvl is phosphorylated and recruits Smurf ubiquitin ligases, which target Pk for degradation (Narimatsu et al., 2009) (Figure 1.7B). Moreover, the Wnt-PCP pathway is directly connected to the actin cytoskeleton (Figure 1.7B). For example, Wnt binding to Fzd receptors promotes Dvl interaction with dishevelled associated activator of morphogenesis 1 (Daam1), a formin protein, and the Rho GEF (WGEF, weak-similarity GEF) that in turn activate the RhoA/ROCK pathway (Gao and Chen, 2010). Upon Wnt stimulation,
Dvl also binds Dvl-associating protein with a high frequency of leucine residues (Daple), which promotes the association of Dvl with aPKC and consequently Rac activation (Ishida-Takagishi et al., 2012). In addition, Wnt association with Ryk and Ror2 receptors triggers activation of
Src and JNK respectively (Angers and Moon, 2009; Gao and Chen, 2010; Nomachi et al., 2008).
The other noncanonical Wnt pathway, the Wnt-Ca+2 pathway, is less understood but may be part of a large signalling network with the Wnt-PCP pathway since regulation of intracellular calcium is critical for CE movements in vertebrates (Veeman et al., 2003; Wallingford et al.,
47
2001a). Activation of the Wnt-Ca+2 pathway, through Fzd and Ror2 receptors, triggers the release of intracellular calcium and subsequent activation of calcium-sensitive proteins such as calmodulin-dependent protein kinase II (CAMKII) and PKC (Angers and Moon, 2009) (Figure
1.7C).
LRP5/6 Ryk Ror2 A B Vangl Vangl C Fzd Fzd Fzd Wnt Wnt ECM Wnt Wnt Wnt PM P Axin G Dvl G G APC GSK3 P PAR6 P Daple Dvl Dvl Dvl Dvl CK1 FLNa Cdc42 WGEFDaam Src PLC P Daple PAR6 Dvl Dvl APC Pk JNK Axin Smurf aPKC GSK3 RhoA -cat IP3 + DAG CK1 Rac1 Cytosol ROCK [Ca+2] PKC