“PHYTOCHEMICAL SCREENING ON THE CONSTITUENTS OF RUMEX OBTUSIFOLIUS” Ph.D Thesis
By ABDUL KHABIR KHAN
Institute of Chemical Sciences, Gomal University, Dera Ismail Khan, Pakistan. 2017
“PHYTOCHEMICAL SCREENING ON THE CONSTITUENTS OF RUMEX OBTUSIFOLIUS” Thesis submitted for the fulfillment of the degree of DOCTOR OF PHILOSOPHY IN CHEMISTRY BY ABDUL KHABIR KHAN
Institute of Chemical Sciences, Gomal University, Dera Ismail Khan, Pakistan. 2017
CONTENTS
DEDICATION i
ACKNOWLEDGMENTS ii
SUMMRY iii
S.No DESCRIPTIONS Page 1 Chapter No 1: Introduction 1 1.1 Importance of medicinal plants 2 1.2 Family Polygonaceae 5 1.2.1 Botany of the family Polygonaceae 6 1.2.2 Chemistry of family Polygonaceae 6
1.2.3 Pharmacology of the family Polygonaceae 7
1.3 Genus Rumex 8
1.3.1 Distribution of genus Rumex 8
1.3.2 Morphology of genus Rumex 14
1.4 Rumex Obtusifolius 16
1.4.1 Habitat 17
1.4.2 Morphology 17
1.4.2.1 Roots 17
1.4.2.2 Stems 17
1.4.2.3 Leaves 17
1.4.2.4 Flower and Inflorescence 17
1.4.2.5 Taxonomic position 18
2 Chapter 2: Literature Review 19
2.1 Traditional uses of Rumex species 20
2.2 Traditional medicinal uses of Rumex species 21
2.3 Pharmacological and Biological screening of rumex species 23
2.4 Compound isolated from Rumex species. 29
4.2.1 Structures of the isolated compounds 33 2.5 R. Obtusifolius 46 2.6 Biosynthesis of anthraquinones 47
3 Chapter No 3: Result and Discussion 50 Preliminary phytochemical screeninig (qualitative) of crude extracts of 3.1 R.Obtusifolius 51
Biological Screening of Dichloromethane Sub-fractions of Rumex 3.2 Obtusifolius 53
3.2.1 Antibacterial screening 53
3.2.2. Antifungal screening 55
3.2.3. Cytotoxicity screening 58
3.3. Secondary metabolites from Rumex Obtusifolius 62
3.4. DCM (Dichloromethane) soluble fraction 62 3.5. Structure elucidation of compounds. 63 3.5.1. Obtusifolate A (102) 63 3.5.1.1. UV-Visible and IR of Obtusifolate A (102) 63 3.5.1.2. Mass spectrometry of Obtusifolate A (102) 64 3.5.1.3. 1H-NMR spectrum of Obtusifolate A (102) 64 3.5.1.4. 13C NMR spectrum of Obtusifolate A (102) 65 3.5.1.5. Other chemical tests for identification Obtusifolate A (102) 65 3.5.2. Obtusifolate B (103) 67 3.5.2.1 UV-Visible and IR of Obtusifolate B (103) 67 3.5.2.2 Mass spectrometry of Obtusifolate B (103) 68 3.5.2.3 1H-NMR spectrum of Obtusifolate B (103) 68 3.5.2.4 13C NMR spectrum of Obtusifolate B (103) 69 3.5.2.5 Other chemical tests for identification Obtusifolate B (103) 69 3.5.3. Obtusifolate C (104) 71 3.5.3.1 UV-Visible and IR of Obtusifolate C (104) 71 3.5.3.2 Mass spectrometry of Obtusifolate C (104) 72
3.5.3.3 1H-NMR spectrum of Obtusifolate C (104) 72 3.5.3.4 13C NMR spectrum of Obtusifolate C (104) 72 3.5.3.5 Other chemical tests for identification Obtusifolate C (104) 73 3.5.4. Obtusifolate D (105) 75 3.5.4.1 UV-Visible and IR of Obtusifolate C (104) 75 3.5.4.2 Mass spectrometry of Obtusifolate C (104) 75 3.5.4.3. 1H-NMR and 13C-NMR spectra of compound D (105) 76 3.5.4.4. Other chemical tests for identification Obtusifolate C (104) 76 3.6. Free radical scavenging activity of the isolated compounds 78 4 Chapter No 4: Experimental 80 4.1. Plant collection, Identification and Grinding 81 4.2. Extraction and Fractionations 81 4.3. Preliminary qualitative phytochemical analysis 81 4.3.1. Alkaloids 81 4.3.2. Flavonoids 81 4.3.3. Tannins 82 4.3.3. Tannins 82 4.3.4. Cardiac glycosides 82 4.3.5. Anthraquinones 82 4.3.6. Steroids 82 4.3.7. Saponins 83 4.4. Sub-fractionation of Dichloromethane soluble fraction 83 4.5. Biological Screening of Dichloromethane Sub-fractions of Rumex 85 Obtusifolius 4.5.1. Antibacterial screening 85 4.5.2. Antifungal screening 85 4.5.3. Cytotoxic screening 86 4.6. Secondary metabolites from R. Obtusifolius 87 4.6.1. Instrumentation 87 4.6.2. Chromatography 87
4.6.3. Isolation, Purification and Characterization of compounds 88 4.6.4. Obtusifolate A (102) 91 4.6.5 Obtusifolate A (103) 93 4.6.6 Obtusifolate C (104) 95 4.6.7 Obtusifolate D (105) 96 4.7. Free radical scavenging activity (RSA) of the isolated compounds 97 5 Chapter No 5: References 99
TABLES
Table No Table Name Page
1.1 Rumex species 9
2.1 Compound isolated from Rumex species. 29
Preliminary qualitative phytochemical analysis of crude extracts of 3.1. 52 R.Obtusifolius
Antibacterial screening of the sub- fractions of DCM fraction of Rumex 3.2 54 obtusifolius (in mm)
3.3 % Inhibition of fungi of sub-fractions of DCM fraction of Rumex Obtusifolius 56
Illustration of percentage mortality of brine shrimps at different 3.4. 58 concentrations of sub-fractions and respective LD50 values
3.5 1HNMR and 13CNMR data of Obtusifolate A(102) (δ=chemical shift in ppm) 66
3.6 1HNMR and 13CNMR data of Obtusifolate B(103), (δ=chemical shift in ppm) 70
3.7 1HNMR and 13CNMR data of Obtusifolate C(104), (δ=chemical shift in ppm) 74
3.8 1HNMR and 13CNMR data of Obtusifolate D(105), (δ=chemical shift in ppm) 77
Percentage of RSA of compounds 102, 103, 104 and 105 from Rumex 3.9 78 Obtusifolius
4.1 Sub-fractionation of Dichloromethane soluble fraction 84
FIGURES AND SCHEMES
Figure and scheme Page
Scheme 2.1:Polyketide pathway for anthraquinone biosynthesis 48
Scheme 2.2:Shikimate pathway for anthraquinone biosynthesis 49
Fig 3.1. % Inhibition of fungi of sub-fractions of DCM fraction of 57 Rumex obtusifolius
Fig No: 3.2. Illustration of percentage mortality of brine shrimps at 60 different concentrations of sub-fractions.
Fig 3.3. Illustration of respective LD values of brine shrimps at 50 61 different concentrations of sub-fractions
Fig 3.4 % DPPH inhibibition zone of compound the four isolated 79 compounds from Rumex Obtusifolius
Scheme 4.1 Extraction and Fraction of R. obtusifolius 89
Scheme 4.2 Chromatographic resolution on Si-gel column eluted 90 with n-hexane, DCM and EtOAs as solvent system.
Dedication Dedicated to my parents (Late) and brothers, their foresight, unconditional support and values paved the way for a privileged education.
Acknowledgements
First of all I bow down my head to the Omnipotent, the most Merciful, the Compassionate, and the Omniscient Al-Mighty ALLAH, whose clemency resulted into my success. I wish to pay homage to the most perfect personality of the world Hazrat Muhammad (PBUH), who enlightened our minds to recognize our Creator.
Firstly I would like to express my feelings of gratitude for the kind support and persistent encouragement of my ever smiling supervisor Dr. Shafiullah Khan. I am very thankful to him for his kind, cool calm and nice behaviour.
I am pleased to acknowledge Dr. Shafiullah Khan, Director of the Institute of Chemical Sciences for providing me with all the facilities to complete this task. Due to his tremendous efforts and dynamic effort for research facilities the Institute is now progressing day by day and the institute which was formerly Department of Chemistry got the name of institute of chemical sciences.
I would also like to acknowledge the contributions of Dr. Kamran khan, Dr. Syed Badsha, Dr. Saed Ahmad and Dr. Hidayat Ullah for their encouraging and supporting behavior.
I am extremely thankful to Dr. Afzal Shah (Chairman Chemistry Department UST Bannu) for providing lab space and Dr. Mushtaq Ahmad (Assistant Prof. UST, Bannu) for helping me in carrying out the biological activities. I am extremely thankful to Beijing University of Chemical Technology China for helping in characterization of the compounds.
I like to express my gratitude to friends especially, Dr. Farman ullah khan and Mr. Fada Khan for their nice company and kind support during the study.
Thanks to all technical and non-technical staff of the Department of Chemistry especially to Hafiz Aziz and Dr. Naqeeb Ullah for their assistance. Also, thank you to all the academic staff.
ABDUL KHABIR KHAN
Summary
The present Ph.D. thesis deals with the phytochemical screening on the constituents of Rumex
Obtusifolius.
Rumex obtusifolius is commonly known as ‘broad-leaf dock’. Itis perennial Herb that grows to a height of 50 to 130 cm. R. obtusifolius occurs along with its very close relative’s R. longifolius and R. crispus. It is widely distributed in ditches, wetlands, riparian areas, roadsides, meadows, waste grounds, disturbed damp areas and pasture fields.
This plant is very important in research point of view because of its traditional uses in medicine in several countries of South America. According to folk medicine this plant’s root has a prominent detoxifying result on the liver and is used against fever, jaundice, and as an anti- anemic tonic. The roots are also laxative. In addition, the leaves of this Rumex are used against hepatic, dermatological and eye problems. They are functional in the relief of furuncles, bruises and are also used as antiseptic and as scar healer. It is used as an antidote to nettle, astringent, depurative, tonic and laxative. It is also used for treatment of tumors, blisters, sores, burns and cancer.
The thesis is presented in following two parts.
Part-A: Biological screeing
The present study has been carried out to investigate the antibacterial, antifungal and cytotoxic screening of sub-fractions of dichloromethane. The bioactivity screening of F1, F2, F3, F4, F5 and
F6 sub-fractions of dichloromethane of R. obtusifolius were assessed using conventional disc diffusion method, agar tube dilution method and the brine shrimp lethality assay. The most
remarkable antibacterial activities are observed with the F6having zone of inhibition (22.5mm) against ampicillin-resistant Escherichia coli. The antifungal results indicate that F3, F4 and F5 inhibited fungal growth more competently as compared to F1 F2 and F6. Maximum inhibition was recorded by F4 (69.4 %) against Aspergillus flavas. F1 does not show any prominent inhibition
(7.4 ± 2.51 to10.3 ± 2.21) against all fungal strains, b/c the probability of bioactive compounds in F1 is less, as ethanolic crude was already extracted with n-hexane in solvent extraction process. LD50 values of cytotoxicity indicate that F4 sub fraction of dichloromethane fraction is the most effective (LD50 =437.4), having 66.65 % maximum mortality of brine shrimp at 100 ppm,while least effective one is fraction of Rumex obtusifolius at early vegetative stages for seeking bioactive sub-fractions.
Part-B: Isolation and Characterization
Phytochemical studies on DCM fraction of R. obtusifolius have resulted in the isolation and characterisation of four new compounds for the first time.
New compounds
1. 1, 8-dihydroxy-5-methyl-3-(4'-(5''methylbut-4''-enoyl)-2'-(2''oxopropyl)-6-tert-pentyl-
anthraquinone-2-carboxylate (Obtusifolate A)(102)
2. 1, 8-dihydroxy-5-methyl-3-(2'methyl-4'-(2''methylbut-1''-enoyl)-6-tert-pentyl-
anthraquinone-2-carboxylate (Obtusifolate B)(103)
3. Ethyl 2-(18,18- dimethylbutanoyl)-1-methyl9,10-dioxo-5-(2-oxopropyl) anthraquinone-
7-carboxylate (Obtusifolate C)(104)
4. Ethyl 2-(16,16-dimethylbutanoyl) -4-methoxy, -1-methyl 9,10-dioxo, anthraquinone-7-
carboxylate (Obtusifolate D)(104)
19 O OH O OH
21 18 17 1 9a 9 8a 8 O 13 6' 3 6 4a 10 10a 16 1' 5 12
4' 2' O 11 14 1'' 4'' H 5'' 2'' O 3'' Obtusifolate A (102) 7'' 6'' O 8''
O OH O OH 18 1 9 8 O 17 9a 8a 13 6' 3 6 10 10a 4a 16 1' 5 12
4' O 11 14 3' 7' 1'' Obtusifolate B (103) O 2'' 4'' H 3''
5'' O 23 O 8 1 21 13 17 7 8a 9 1a O 11 18 20 12 19 O 3 5a 10 4a 5 4
O 14 O 15 Obtusifolate C(104) 16
O 21 O 8 1 19 13 8a 9 1a O 15 11 7 16 18 12 17 O 3 5a 10 4a 5 4 Obtusifolate D (105) 14 O O
Chapter No 1
Introduction
1
1.1. Importance of medicinal plants
Local plant derivatives play a key role in the provision of medical care for human beings all over the World. The reason which compels people to use wild plants species as foodstuff is times of famine, however on the other hand eating plant derivatives is becoming a fashion in our modern culture [1]. Plants and their derivatives are getting more importance against many diseases due to their no or less side effects and non-toxic nature. So, scientists have been constantly studying on the identification, analysis, investigation, characterization and assessment of medicinal plants [2,
3]. Approximately 0.4 billion people at present time depend on traditional herbal medicine even in the modern world. About 25 percent of standard drugs recommended by physicians originate from folk and traditional medicines still in the present era [4]. People of the developing world have turned back their interest and concentration towards herbal medicines for substitutive health care purposes because they are cheap and easily accessible as compared to synthetic medicines
[5].
Nature has been a source of therapeutic agents for thousands of years and many new drugs have been resulted from natural sources, many of these identifications and isolations were based on the uses of the agents in traditional remedy [6]. In the early 20th century botanical medicine was chief healthcare system as analgesics and antibiotics were not as yet exposed. Botanical medicine slowly lost its attractiveness among the people due to arrival of allopathic system of medicine which is based on the quick curative actions of synthetic medicine [7]. Lately there has been a shift in worldwide tendency from synthetic to botanical medicine, which may be called “Return to Nature”. Medicinal plants have been recognized for millennia and are extremely valued worldwide as a large and rich source of medicinal agents for the prevention of ailments [8]. The search for perfect health and for relieves pain, early man to explore immediate and instant natural
2
products. It brings about for the development of plants, animals and minerals products, as a variety curative agents [9].
Plants have been used as medicines all time during the history. In fact, investigations on wild animals confirm that they eat certain wild plants to care for themselves for some illnesses. The use of botanical medicine is extremely well established and recognized in Asia; therefore the majority of the medicinal plants species that have global recognition come from India and China.
The applications of herbal medicine are increasing rapidly, particularly for correcting imbalances caused by modern diet and lifestyle in N. America and Europe. Most people now days take medicinal plant derivatives on a daily basis, to maintain good health as much as to treat disease
[10]. The importance of traditional health systems and medicinal plants in solving the health problems in world is gaining increasing concentration. Due to this interest, the research on plants of medicinal importance is growing extraordinarily all over the world, frequently to the harm of natural habitats and mother populations in the countries of origin. Most of the developing countries have adopted traditional medicinal practice as a fundamental component of their civilization. The medicinal preparations are resulting from plants, either in the simple form of raw plant materials or in complex form of mixtures and crude extracts etc [11].
In beginning of development of modern medicines, biologically active compounds from higher plants species have showed an important role by providing medicines pain to and combat diseases e.g. In the British Pharmacopoeia in1932; more than seventy percent of organic monographs are on plant derivative products, but with the initiation of antibiotics and synthetic medicines the role of plant derived remedial products much declined especially in the developed countries. Therefore, In the British Pharmacopoeia in (1980), the share of plant-derived monographs fell to about twenty percent. In terms of new chemical entities introduced as
3
remedial agents over the past few decades, the share of herbal-derived medicines has been no
more than two percent [12].
This latest revival of interest and importance in botanical medicines has been spurred on by
several reasons, which are listed below [13-16].
I. The effectiveness of herbal medicines
II. Source of direct remedial agents
III. Model for new synthetic compounds
IV. The preference of patients for natural therapies, a greater interest in alternative drugs and
a commonly held belief that botanical medicines are better to artificial products.
V. The consumption, production and international trade in medicinal plants species are
growing and predicted to grow in future somewhat notably.
VI. A disappointment with the outcomes from modern synthetic products and the idea that
phytomedicines may be useful in the treatment of some diseases where usual therapies
and medicines have verified to be insufficient and poor.
VII. A movement and progress towards self-medication
VIII. The high cost of modern drugs
IX. Side effects of the most modern drugs
Study of the biological activities of plants species for the last two centuries have resulted
compounds for the development and improvement of modern synthetic organic chemistry as a
4
key direction for discovery of more effective novel and useful therapeutic products [9]. There are
2, 50,000 flowering plants are estimated on the earth, in which only six percent have been analyzed for biological activity and about 15 percent have been screened phytochemically, so consistent research study should be carried out to find out a probable abundance of medicinal extracts in these plant species. [17]. Plants contain biologically active agents. For their investigation and analysis, necessary methods and tools are required. These consist of suitable chemical screening procedures and biological activities. To investigate and explore for novel antimicrobial agents is necessary to observe microbial occurrence and resistance of fetal opportunistic infections [18].
Natural products have a broad diversity of functions and structures, and have traditionally provided substantial inspiration for drug development and improvement programs. Modern screening and isolation techniques have enhanced the search for new molecules and increased interest in folk medicinal plant extracts [19].
1.2. Family Polygonaceae
Polygonaceae comprises about 50 genera and 1120 species distributed worldwide, but primarily north temperate with a few species in tropical zones [20].
Secondary metabolites of the families Polygonaceae and Asteraceae species can be considered as promising starting materials for pharmaceutical discoveries, in consequence of their pharmacological potential, and in particular their remarkable anti-inflammatory and antitumour properties, which provides a basis for screening for new active constituents from these families for the treatment of cardiovascular diseases and Cancer [21].
5
1.2.1. Botany of the family Polygonaceae
The family was divided into two subfamilies, Polygonoideae and Eriogonoideae by Brandbyge
(1993) [22]. The largest genera include Rumex, Polygonum, Rheum, Coccoloba, Calligonum and
Persicaria. Polygonaceae is most diverse in the Northern Temperate Zone. Some species of
Persicaria, Fallopia, Rumex and Polygonum are among the most troublesome invasive species in
N. America and Europe [23]. Morphologically its plants are herbs, shrubs, or small trees, sometimes monoecious or dioecious [24].
Most of the species of Polygonaceae family are annual or perennial herbs, some are small shrubs, but trees and vines are rarely present. A distinctive feature of this family is the ocreae, a nodal sheath variously interpreted as an outgrowth of the sheathing base of the petiole, as an expanded axillary stipule, or as connate stipules. The leaves of buckwheat are nearly always alternate and penninerved, rarely whorled or opposite. In most genera the stem is characteristically swollen at the points of nodes. Flowers are generally perfect and actinomorphic with two to six uniform petaloid petals, often in two whorls of three or one whorl of five, persistent in the fruit, the ovule is generally orthotropus, the fruit is a lenticular nut or trigonous, and the seeds contain copious endosperm [22, 23, 25].
1.2.2. Chemistry of family Polygonaceae
The most important compounds isolated from species belonging in the Polygonaceae family are polysaccharides, flavonoids mainly flavonols or their O/C-glycosides (O- glycosides and C- glycosides) and phenylpropanoids particularly caffeic acid and its glycosides, sinapic acid and chlorogenic acid [22-24]. Other important phenolic compounds are anthraquinones particularly physcion, chrysophanol and emodin [25-27] and stilbenes often piceid, trans-resveratrol and its
6
glycoside [22, 23, 28, 29]. Characteristic components of some Polygonum plants are drimane- type norsesqui- and sesquiterpenoids and sulfated flavonoids [30-32]. It is of great interest that
Rumex plants contain 24-norursane-type triterpenoids [33].
The most of the species occurring in the Carpathian Basin have only been poorly analyzed except Fallopia species. Anthraquinones, flavonoids, stilbenes and polysaccharides have been identified from their stems, roots, flowers and leaves [23, 34, 35].
1.2.3. Pharmacology of the family Polygonaceae
Many plants of Polygonaceae are rich sources of bioactive constituents which have a wide range of medicinal properties. Anti-inflammatory, antioxidant, antimicrobial, antitumour, antiulcerogenic and antileukaemic properties and aldose reductase, α-glycosidase, lipid peroxidation and platelet aggregation-inhibitory effects were reported, previously.
The polysaccharides have been found to exhibit significant radical-scavenging properties, representing their potential application as novel natural antioxidants [34]. Stilbene derivatives such as resveratrol and piceid with antifungal and antibacterial activities have also been isolated from many Polygonaceae plants [36]. Chalcones and flavonoids have various biological activities. Their strong antioxidant properties in particular play significant roles against radical oxidative stress causing pathological processes i.e. cancer or arteriosclerosis [37]. Quercetin, isolated and elucidated from many species of this family has the ability to induce apoptosis in human leukaemic cells [38].
A quercetin (quercetin-3-O-β-D-glucuronopyranoside) was identified and isolated in large amount from Rumex aquaticus and has been investigated in many experimental models. It confirmed to inhibit neutrophil infiltration into the gastric mucosa, pro-inflammatory cytokine
7
(IL-1β and TNF-α) production [39], the production of intracellular ERK½ and ROS activation
[40]. It also decreased the area injuries of gastric lesion sizes, the gastric pH and acid output [41].
Its anti-inflammatory and antioxidative properties were evaluated on cultured feline oesophageal epithelial cells [42].
Sesquiterpenes extracted and isolated from P. hydropiper possessed interesting biological properties, i.e. antitumour-promoting, antifungal and lens aldose reductase-inhibitory effects.
[32, 43]. The same species also has tyrosinase-inhibitory, oestrogenic, antimutagenic and antinociceptive properties [44-46].
R.palmatum, among the well-known species of the Polygonaceae, produces anthranoids as the most characteristic compounds. Their pharmacological effects have been studied in many assays.
Aloe emodin induces the apoptosis of human being nasopharyngeal carcinoma cells [47].
Emodin has antitumour and antidiabetic properties [48-50]. Additionally, emodin has been evaluated for its neuroprotective and lipid-lowering activities in rat cortical neurons [51, 52].
1.3. Genus Rumex
The name Rumex derived from the Latin words for dart, alluding to the shapes of the leaves. It is the largest genus of family Polygonaceae [53].
1.3.1. Distribution of genus Rumex
This genus includes more than 250 species distributed worldwide [54]. These species are listed in Table No 1.1.
Rumex plants can constitute a considerable part of the biomass (about 70 % in the mentioned studies) and the yield reduction is directly proportional to the area of ground covered by dock
8
species. The loss in grass growth is caused by competition from the dock plants, mostly by shading but also by below ground competition for nutrients and water [55]. Several investigations confirm that Rumex species can cause reduced grass yields [56, 55].
The population dynamics of Rumex pants in undamaged grassland is an example of the so-called
‘phalanx’ strategy (The strategy of a phalanx species is to remain in a relatively fixed position as long as possible and to gradually colonise neighboring fields) [57].
Table No 1.1. Rumex species
1. Rumex acetosa 121. Rumex acetosella
2. Rumex balcanicus 122. Rumex brownie
3. Rumex densiflorus 123. Rumex dentatus
4. Rumex lorentzianus 124. Rumex x lousleyi
5. Rumex x acutus 125. Rumex albescens
6. Rumex brownie 126. Rumex bucephalophorus
7. Rumex diclinis 127. Rumex digynus
8. Rumex ludovicianus 128. Rumex lugdunensis
9. Rumex x alexidis 129. Rumex alpestris
10. Rumex chrysocarpus 130. Rumex confertus Willd.
11. Rumex dimidiatus 131. Rumex dimorphophyllus
12. Rumex lunaria 132. Rumex luxurians
13. Rumex altissimus 133. Rumex alpinus
14. Rumex conglormeratus 134. Rumex confuses
15. Rumex dobrogensis 135. Rumex dissimilis
9
16. Rumex maderensis 136. Rumex lycheanus
17. Rumex aquaticus 137. Rumex angiocarpus
18. Rumex crispus 138. Rumex costaricensis
19. Rumex dregeanus 139. Rumex dolosus
20. Rumex maritimus 140. Rumex magellanicus
21. Rumex azoricus 141. Rumex aquitanicus
22. Rumex crystallinus 142. Rumex cristatus
23. Rumex drummondii 143. Rumex drobovii
24. Rumex polygamous 144. Rumex polycarpus
25. Rumex dumosiformis 145. Rumex dufftii
26. Rumex flexuosiformis 146. Rumex flexicaulis
27. Rumex gusuleacii 147. Rumex gussonii
28. Rumex promiscuous 148. Rumex polyklonos
29. Rumex ellenbeckii 149. Rumex dumosus
30. Rumex frutescens 150. Rumex foliosus
31. Rumex hayekii 151. Rumex hadmocarpus
32. Rumex pulcher 152. Rumex Propinquus
33. Rumex engelmanni 153. Rumex dumulosus
34. Rumex fueginus 154. Rumex fontanopaludosus
35. Rumex hazslinszkyanus 155. Rumex halophilus
36. Rumex quarrei 156. Rumex protractus
37. Rumex ephedroides 157. Rumex durispissimus
38. Rumex gamsii 158. Rumex foveolatus
10
39. Rumex heimerlii 159. Rumex hararensis
40. Rumex raulini 160. Rumex pseudonatronatus
41. Rumex erosus 161. Rumex ecklonianus
42. Rumex gangotrianus 162. Rumex franktonis
43. Rumex hellenicus 163. Rumex hasslerianus
44. Rumex rechingerianus 164. Rumex pseudopulcher
45. Rumex erubescens 165. Rumex ecuadoriensis
46. Rumex gieshueblensis 166. Rumex fraternus
47. Rumex henrardi 167. Rumex hastatulus
48. Rumex rectinervius 168. Rumex pseudoscutatus
49. Rumex erythrocarpus 169. Rumex elbrusensis
50. Rumex giganteus 170. Rumex fringillimontanus
51. Rumex hesperius 171. Rumex hastatus
52. Rumex recurvatus 172. Rumex pseudoxyria
53. Rumex hymenosepalus 173. Rumex esquirolii
54. Rumex interruptus 174. Rumex ginii
55. Rumex kaschgaricus 175. Rumex heteranthos
56. Rumex ruwenzoriensis 176. Rumex rhaeticus
57. Rumex x impurus 177. Rumex euxinus
58. Rumex inundates 178. Rumex gmelini
59. Rumex kaschmirianus 179. Rumex heterophylus
60. Rumex sagittatus 180. Rumex rhodesius
61. Rumex inconspicuous 181. Rumex evenkiensis
11
62. Rumex iseriensis 182. Rumex gombae
63. Rumex kerneri 183. Rumex hexagynus
64. Rumex sagorski 184. Rumex x romanicus
65. Rumex integer 185. Rumex exspectatus
66. Rumex jacutensis 186. Rumex gracilescens
67. Rumex khekii 187. Rumex hippiatricus
68. Rumex salicetorum 188. Rumex romassa
69. Rumex integrifolia 189. Rumex fallacinus
70. Rumex japonicas 190. Rumex gracilipes
71. Rumex khorasanicus 191. Rumex hirsutus
72. Rumex salicifolius 192. Rumex rosemurphyae
73. Rumex intercedens 193. Rumex fascicularis
74. Rumex johannis-moorei 194. Rumex graminifolius
75. Rumex knafii 195. Rumex horizontalis
76. Rumex salinus 196. Rumex roseus
77. Rumex intermedius 197. Rumex fascilobus
78. Rumex kamtshadalus 198. Rumex granulosus
79. Rumex komarovii 199. Rumex hoschedei
80. Rumex samuelssoni 200. Rumex rossicus
81. Rumex krausei 201. Rumex fimbriatus
82. Rumex marschallianus 202. Rumex griffithii
83. Rumex obovatus 203. Rumex hostilis
12
84. Rumex sanguineus 204. Rumex rothschildianus
85. Rumex lachanus 205. Rumex finitimus
86. Rumex maximus 206. Rumex x grintzescui
87. Rumex obtusifolius 207. Rumex hultenii
88. Rumex sanninensis 208. Rumex rugosus
89. Rumex lacustris 209. Rumexhungaricus
90. Rumex megalophyllus 210. Rumex hybridus
91. Rumex occidentalis 211. Rumexhydrolapathum
92. Rumex suzukianus 212. Rumex rupestris
93. Rumex leptocaulis 213. Rumex lanceolatus
94. Rumex monistrolensis 214. Rumex meyeri
95. Rumex oxysepalus 215. Rumex occultans
96. Rumex nankingensis 216. Rumex vesceritensis
97. Rumex leptophyllus 217. Rumex langloisii
98. Rumex montanus 218. Rumex mezei
99. Rumex pakistanicus 219. Rumex ochotensis
100. Rumex natalensis 220. Rumex vesicarius
101. Rumex limoniastrum 221. Rumex lanuginosus
102. Rumex monticola 222. Rumex microcarpus
103. Rumex pallidus 223. Rumex orbiculatus
104. Rumex neglectus 224. Rumex violascens
105. Rumex linearis 225. Rumex lapponicus
106. Rumex muelleri 226. Rumex microdon
13
107. Rumex palustris 227. Rumex orientalis
108. Rumex nematopodus 228. Rumex wachteri
109. Rumex lingulatus 229. Rumex lanuginosus
110. Rumex munshii 230. Rumex mirabilis
111. Rumex palustroides 231. Rumex orthoneurus
112. Rumex nemorosus 232. Rumex weberi
113. Rumex litoralis 233. Rumex latifolius
114. Rumex muretii 234. Rumex mixtus
115. Rumex pamiricus 235. Rumex oryzetorum
116. Rumex nepalensis 236. Rumex longifolius
117. Rumex lonaczewskii 237. Rumex lativalvis
118. Rumex muricatus 238. Rumex moedlingensis
119. Rumex pannonicus 239. Rumex osswaldii
120. Rumex nervosus 240. Rumex longisetus
1.3.2. Morphology of genus Rumex
Rumex plants belong to the hemicryptophytes. Characterizing for this group, which includes many rosette plants and grasses, is that buds are positioned at the soil surface, protected by leaf and stem bases [58].
Plants of Rumex are perennials, biennials or annuals, mostly herbs, rarely shrubs. Leaves are usually alternate, occasionally sagittate or hastate. They have long fleshy roots, rarely the roots
14
are rhizomatous. Flowers are generally unisexual or hermaphrodite arranged in whorls on branched or simple in florescences. In most members of Rumex the flowers are green, however in some species like Rumex acetosella the stems and flowers are brick-red. Typically fruits are trigonous nuts [59].
15
1.4. Rumex obtusifolius
https://en.wikipedia.org/wiki/Rumex_obtusifolius and picture taken from my own mobile Q-LT700
16
1.4.1. Habitat
It is commonly known as ‘broad-leaf dock’ [60]. Rumex is a pliny name for sorrel while the meaning of Obtusifolius is ‘obtuse leaved’ [61].
Ditches, wetlands, riparian areas, roadsides, meadows, waste grounds, disturbed damp areas and pasture fields. [62] In Sweden R. obtusifolius occurs along with its very close relative’s R. longifolius and R. crispus. [63]
1.4.2 Morphology
Rumex obtusifolius is perennial Herb that grows to a height of 50 to 130 cm. Its morphology is listed below [54, 64].
1.4.2.1 Roots
Brown -black, vertical, large, up to 2.5 cm in diameter.
1.4.2.2 Stems
Erect, 30-60 cm, branched, grooved. It is branched above middle or in upper 2/3 and glabrous.
1.4.2.3 Leaves
Basal leaves; leaf blade oblong, 5-20 × 3-8cm, petiole 3-4 cm, both surfaces glabrous, midvein prominent abaxially, base subcordate or rounded , apex acute or obtuse, margin somewhat undulate. Cauline leaves small; shortly petiolate, ocrea fugacious.
1.4.2.4 Flowers and Inflorescence
Flowers are bisexual and dense. Inflorescence is broadly paniculate and large.
17
1.4.2.5 Taxonomic position
Kingdom: Plantae
Unranked: Angiosperms
Unranked: Eudicots
Unranked: Core eudicots
Order: Caryophyllales
Family: Polygonaceae
Genus: Rumex
Species: Rumex Obtusifolius
18
Chapter No 2
Literature Review
19
Many species of genus Rumex have been used as vegetables and for their medicinal importance.
Based on the traditional data and knowledge, different pharmacological and phytochemical studies have been at the focus of researchers. The aim of this chapter is to collect information of the recent state of knowledge of local and traditional medicinal values, pharmacological properties and chemical constituents, in order to identify the therapeutic potential of Rumex species and further directions and guidelines of research study.
A numerous ethnopharmacological and ethnobotanical literature reports regarding to the traditional uses and occurrence of Rumex species is present. [65-67].
2.1. Traditional uses of Rumex species
Rumex species are used traditionally as edible plants in many parts of the World. In some regions of world the leaves of Rumex species for example Rumex vasicarius, Rumex crispus, Rumex acetosella, Rumex abyssinicus, Rumex singuineus, Rumex acetosa Rumex tuberosus and Rumex thirsiflorus are used as foods mostly in the forms of salads and sauces [68-75]. The airborne portions of many plants e.g. Rumex acetosella, Rumex acetosa, Rumex crispus, Rumex pseudonatronatus & Rumex patientia are gathered mostly in the spring season and used as vegetables [69, 76, 77]. In majority cases, the roots are used for treatment, while the other parts, such as the fruits, seeds and leaves are also applied. Leaves are used for soups, sauces and dressed with olive oil. Sometime leaves are mixed with boiled potatoes to moderate their PH [70,
72, 74, 76, 78]. Some members of Rumex are consumed fried in olive oil or lard or sautéed with butter or are used as filling for pie (Rumex alpinas, Rumex acetosa, Rumex nepalansis and
Rumex acetosella) [79-82]. In N. America R. hymenosepalus’s roots are used as chewing gum
[79, 83], While the stems of R. alpinus and R. acetosa are used as raw snacks [72, 79, 84]. In
20
some parts of India nearly all parts of R. crispus are consumed as medicine and also as food. The extremely young leaves of this species are cooked as a potherb or added to salad and soup.
Sometime stems are peeled and the inner parts are eaten. The flour which is made from dry seeds of the said plant can be used as for making pancakes [85].
In many parts of alpine, R. alpinus was used in past for different purposes, e.g. stem was peeled and applied instead of rhubarb, put into cakes, puddings and biscuits or eaten fresh [86]. The leaves of some Rumex species for example that of R. acetosa is used for making sarma i.e. a traditional south-Eastern and Middle Eastern food [87]. The tuberous roots of R. abyssinicus are
applied to purify butter s and give it a yellow colour [88]. Furthermore, rhizomes the of some species (R. hymenosepalus, R. abyssinicus) have been used in North America & Kenya as a source of a yellow stain which renders cellulose fibers red-brown when applied in the presence of sodium carbonate (Na2CO3) [79, 89]. Several species of genus Rumex are cultivated like
Rumex vasicarius & Rumex acetosa [90].
2.2. Traditional medicinal uses of Rumex species
The airborne parts, roots and leaves of the plant species are used in traditional medicine for the cure of several diseases e.g. infections, constipation, mild diabetes, diarrhoea, jaundice, oedema, inflammation and as an analgesic antihypertensive and diuretic. These parts are also used for the treatment of skin, liver and gallbladder diseases. The genus Rumex has attracted the concentration of many scientists and investigators due to its medicinal importance and phytoconstituents. The various crude extracts of this genus species, and compounds extracted and isolated from them, have been verified to possess various pharmacological properties, such as antioxidant, antiinflammatory, antibacterial, antitumour, antifungal properties and antiviral in
21
vivo and in vitro [28, 29,39, 91-95]. Local and traditional names for many species used as food reveal their gustatory properties, aroma. Due to gentle laxative effect of the roots of many plants of Rumex, they have been used in medicines from ancient time. R. acetosa is present in the
Korean Food Code (Korea Foods and Drugs Administration) as one of the key food resource and has been used in folk medicine as a mild purgative & also for the treatment of cutaneous diseases
[96].
For medicinal purposes mostly infusions or decoctions are prepared from the various parts of rumex plant e.g. the young leaves of R. nepalensis forms tinging nettles by rubbing over the affected parts after injury [94].
There is an old verse about R. obtusifolius. “Nettle in, dock out. Dock rub nettle out!” there is no objective proof which supports this rhyme aside from the reality that firm rubbing (by itself) was found to create a short-lived reduction of the pain inflicted by nettle. It is also possible that the
effort times and spent on finding a dock (R. Obtusifolius) leaf is enough for distracting the victim s from the itching caused by nettle rash [97, 98].
Various parts of Rumex alpinus, Rumex acetosella, Rumex acetosa, Rumex confertus, Rumex obtusifolius and Rumex crispus are mainly used in Europe to treat of various diseases. These species are also used for the treatment of diarrhoea, constipation, swellings, sores, kidney disorders and rashes and as an astringent in Romania and Hungary [76, 99].
In Ireland and England R. acetosa is applied for warts, scurvy, wounds, bruises, sore throat and jaundice .Furthermore, R. hydrolapathum, R. palustris and R. conglomeratus are also used for the treatment of scurvy, as “blood purifier”, for sunburn. They are also used for cancer therapy and bathing rashes. The decoctions of the seeds of R. obtusifolius are applied against all kinds of
22
coughs, bronchitis and colds [100]. In Turkey Rumex alpinus is used to treat diarrhoea, constipation and eczema and in Bulgaria and Ukraine this plant is used for the treatment stomach diseases and as a laxative [86].
Rumex alpinus roots and leaves have been used in traditional medicine in Austria and to treat viral diseases [101]. R. nervosus is used as a medicinal species for the treatment of acne, as an ophthalmic antiseptic agent and as a hypoglycaemic agent. It is also applied for the cure of eczema, wounds and rabies [102].
In Pakistan R. crispus is used for the treat of cough, constipation, Skin problems, rheumatism and tonic [103].
2.3. Pharmacological and Biological screening of Rumex species
A number of crude extracts and isolated compounds have been screened for their antioxidant, antibacterial and antitumor properties. The antifungal, antiviral, antiulcerogen, hepatoprotective, antidiabetic, purgative, anthelminthic, anti-inflammatory, antiplasmodial and antifertility, properties have also been evaluated. A detail of the biological activities performed on various species of Rumex is listed below.
The antioxidant properties of thirty medicinal species of Rumex that used in Mexico were evaluated. The powder plant materials were extracted with water by heating (85°C) for ten minutes. Two-stage Trolox-based assay analysis showed that the extracts of the stem of R. hymenosepalus had significant activity [104]. The antioxidant activities of traditional medicinal species of Cameroon were evaluated by hemoglobin ascorbate peroxidase activity inhibition
(HAPX), the Trolox equivalent antioxidant capacity and DPPH bleaching methods. The result confirmed that R.abyssinicus has the greatest activities in all the assays. In DPPH method, the
23
area under the kinetic curve was 10. Gallic acid was added as standard instead of trolox in TEAC assay. Gallic acid equivalent antioxidant capacity (GEAC) was 50 μg/cm3 for R. abyssinicus. In
HAPX assay the inhibition of the ascorbic acid consumption of R. abyssinicus was 100% [105].
Lone etal in 2007 evaluated the antioxidant potential of an ethanol extract of R. patientia revealed its strong activity. The extract scavenged DPPH radicals significantly and dose-
3 3 3 dependently {O2 (IC50 =29 μg/cm ), NO (IC50 =33 μg/cm ) and OH radicals (IC50=63 μg/cm )}.
Its total polyphenols content calculated in gallic acid equivalent was 315 mg/g [106]. The antioxidant study of orcinol and flavans (anthraquinones) isolated from R. patientia showed that just catechin and 6-chlor-ocatechin have strong DPPH radical scavenging activity. In this study
TLC plate was sprayed with a 0.2% DPPH solution in MeOH after developing and drying.
Active compounds appeared as yellow spots on a purple background [92].
The total phenolic content, reducing power and antioxidant activity and of hexane, EtOH,
CHCl3, EtOA and aqueous extracts of the stems, leaves and seeds of R.japonicus were studied by
DPPH assay, using superoxide radical and β-carotene bleaching method. The ethyl acetate fraction has strong antioxidant activity (Superoxide radicals scavenging activity=16.4±1.44ppm
3 3 and DPPH radical scavenging activity=86.0±0.20 μg/cm , EC50=0.04±10.0001 μg/cm ), which linked with the high content of phenolic compounds, especially pyrocatechins and pyrogallols
[107]. An investigation was performed with R. pulcher and R.papillaris and recognized that the
3 3 radical scavenging activity of the said plants were EC50=02.45 mg/cm and 03.31mg/cm , the reducing power developed as 0.60 mg/cm3 and 0.80 mg/cm3and the β-carotene bleaching inhibition were 0.30 mg/cm3 and 0.34 mg/cm3 respectively [108]. R. vesicarius extracts (MeOH acetone and EtOA and) were tested on different methods i.e. lipid per oxidation and DNA-sugar damage inhibitory activity, hydrogen peroxide scavenging effect and DPPH radical. In each case
24
the methanol extract of the showed the maximum inhibitions, 33.80%, 66.30% and 96.60% lipid per oxidation, DNA–sugar damage, and DPPH radical scavenging respectively [109]. The antioxidant properties of crude extracts (MeOH, hexane, EtOH, CHCl3, BuOH and H2O) of R. hastatus were examined, and the total flavonoid and phenolic contents were also investigated.
The BuOH and MeOH extracts showed the highest activities in all except H2O2 radical scavenging assay, where the CHCl3 extract showed strong activity[110].
An antioxidant study of water and acetone extracts of R. hastatus was performed with different assays like OH-radical scavenging, DPPH, ferric ion, total antioxidant capacity and reducing power. The results proved that both extract had moderated activities [111]. Ethanol, ether, and hot aqueous extracts of the seeds and leaves of R. crispus were investigated pharmacologically, the water extracts showed the higher antioxidant activities than the others, while total phenolic contents was highest in the EtOH extract of the seeds (220.0 μg/500 μg extract). In case of DPPH scavenging activity and reducing power, the EtOH extract of the seeds showed potential activities [112]. The singlet oxygen quenching abilities and the protective properties of n-hexane, chloroform, ethyl acetate and butanol extracts of R. crispus seeds against photodynamic damage were studied in biological system. High levels of total phenol contents were seen for the EtOA
3 3 and BuOH (QC50=82 μg/cm for EtOA and QC50=116 μg/cm for BuOH) which were somewhat
3 similar to that of the positive control ascorbic acid (QC50 =86 μg/cm [113].
The MeOH extract of R. crispus roots showed strong DPPH radical scavenging property
3 +3 (IC50=42.86 μg/cm ). Therefore, it has a significant ability to guard against H2O2/Fe /ascorbic acid-induced protein damage [114]. The free radical DPPH scavenging activity EtOH extract of
R. dentatus showed a higher activity (96%) than MeOH extract (73%). The ascorbic acid
(positive control) displayed 95% scavenging potential. The in vitro inhibition of LP was 86%
25
(ethanol extract) and 78% (methanol extract) [115]. The antioxidant potential of acetone and water extracts of R. dentatus was examined with different methods like DPPH, Fe+3 reducing power, OH radical scavenging, and total antioxidant activity. The results showed that both of the extracts have moderate antioxidant property [111]. A lyophilized extract of R. induratus leaves
3 showed a concentration-dependant antioxidant potntial (IC50=149.90 μg/cm ). Furthermore, this
3 extract exhibited inhibitory effects on XO (IC25 =708.80 μg/cm ) [116]. Another investigation proved that a lyophilized aqueous extract of R. induratus leaves had a strong concentration-
3 dependant antioxidant property with IC50 value of 106.50 μg/cm . It also showed significant
3 scavenging effects against NO free redical (IC50=92.70 μg/cm ) [78].
The cytotoxic activities of EtOH extracts of the roots, leaves and fruits of Rumex acetosella,
Rumex acetosa, Rumex confertus, Rumex crispus , Rumex hydrolapathum and Rumex obtusifolius
were studied against the 2 humans leukaemic cell lines 1301(human Tlymphoblastic cells) and
EOL-1(humans eosinophilic leukaemia) and the normal H9 (a clonal derivative of the T cell line).
3 The IC50 values exposed that R. confertus showed the highest activity 0.220 mg/cm (1301) and
3 0.230 mg/cm (EOL-1)] for roots. The leaves extracts of R. obtusifolius IC50 values were 0.47mg/ cm3 (1301) and 0.44 mg/ cm3 (EOL-1), while for R. hydrolapathum were 0.420 mg/cm3 (1301) and 0.170 mg/cm3 (EOL-1)] for fruits extracts [117].
The antiproliferative properties of water and various organic solvent extracts of twenty seven
plants species belonging to Polygonaceae (Rumex) were investigated against humans tumour cell lines (MCF-7, A-431 and HeLa) by performing the MTT assay. The chloroform extract of R. aquiticus (60.90% at30 μg/cm3 on HeLa cells and 69.30% at30 μg/cm3 on MCF7cells), R. acetosa (77.70% and 97.00% at10 and 30 μg/cm3 on HeLa cells), R. scuitatus (51.20% at 30
μg/cm3 on HeLa cells and 56.20% at 30 μg/cm3 on MCF7cells) and R. thirsiflorus (96.20% at 30
26
μg/cm3 on A431cells and 88.55% at 30 μg/cm3 on MCF7cells) showed considerable cell growth inhibitory effects against one or more cell lines [118]. In a previous research, Rumex patientia
3 was proved to have strong cytotoxic property against brines hrimp(LC50=1.3 mg/cm ) [119]. The
cytotoxic property of R. obtusifolius extract was screened by brine shrimps lethality assays. The
3 3 LD50 values of DCM (1.00 mg/cm ) and MeOH (41.00 mg/cm ) extracts revealed that this species has comparative low cytotoxic effects with the positive control podophyllotoxin [120].
Demirezer etal performed cytotoxicity screening on human breast carcinoma (MCF), humanmelanoma (HM02) and human epidermoid carcinoma (HEPG2) cell lines. In this study, anthraquinones (compounds No 1-3), flavans (51, 53) andorcinol (85) isolated from R. patientia
were examined. The result showed that none of the isolated compounds inhibited the growths of the cell lines [92]. Whereas anthraquinone aglycones (1–4) from R.scutatus proved to possess potent cytotoxic activities [LC50=0.05 mg/cm3 (1); 0.06 mg/cm3 (2); 0.15 mg/cm3 (3) and 0.01 mg/ cm3 (4)]. Catechin (51) and anthraquinone glycosides were inactive [92].
The antiproliferative properties of torachrysone-8-glucosides, nepodin-8-glucoside and chrysophanol were tested on MCF-7, 7901(gastriccancer), SKOV-3(oophoroma) and
A375(melanoma) tumour cell lines, the results indicated that compound No 2 showed higher activity(IC50=20.4 μM on MCF7,513 μM on7901,83.1 μM on A375 and 5.62 μM on SKOV-
3cells), than the naphthalene compounds [121]. Emodin (1) is proved to be as a atyrosine kinase inhibitor [122]. The tumour inhibitory property of Emodin (1) is based on the mammalian cells cycle modulation in definite oncogene-overexpressing cell [123].
A cytotoxic activity of emodin, emodin-8-O-β-D-glucopyranosides, emodin-8-O-β-D-(6′-O- acetyl)gluco-pyranoside, chrysophanol, physcion , citreoresin, , chrysophanol-8-O-β-D-(6′O-
27
acetyls) glucopyranoside, chrysophanol-8-O-β-D-glucopyranosides, aloesin, nepodin-8-O-β-D- glucopyranoside, nepalensides A and B, orcinol glucoside, hastatuside A, orientaloside,
torachrysone, torachrysone-8-O-β-D-glucopyranosides, rumexneposides A and B, hastatuside B,
(–)-epicatechin, (–)-epicatechin-3-O-gallate, lyoniresinol3α-O-β-D-A. glucopyranoside, and
(3,5-dimethoxy-4-hydroxyphenols)-1- O-β-D-(6-O-galloyl)-glucoses, isolated from R. hastatus and R. nepalensis was investigated against H522 (lungcancer), A549, MCF-7, MCF-10A and
SKBR3 cancer cell lines by performing the MTT method, with cisplatin as positive control.
Among these compounds chrysophanol-8-O-β-D-(6′O-acetyl)glucopyranoside, orientaloside and rumexneposides A, and exhibited marked activities [95].
28
2.4. Compound isolated from Rumex species.
The record of previously isolated compounds from Rumex species is listed in table No 2.1.
Table No 2.1. Compound isolated from Rumex species.
S. Name Reference No Basic skeleton No 1 Emodin 2 Chrysophanol 89,28,92,94,124,2 3 Physcion 6,27, 125, 126 4 aloe-emodin 5 Citreoresin 6 Rhein 121 7 Endocrocin 95
8 emodin-6-O-β-D-glucopyranosides 127
9 emodin-8-O-β- D-glucopyranosides 128 10 Ziganein 129, 130 11 Przewalsquinone 12 Barbaloin 127 Antraquinones 13 Rumexone 130 14 rumejaposide A(10R) 131,132,133 15 rumejaposide B(10S) 16 rumejaposide C(10R) 17 rumejaposide D(10S) 18 rumejaposide E(10R) 19 rumejaposide F(10S) 20 patientoside A(10S) 21 patientoside A(10S) 22 Dianthrones of chrysophanol 26, 127 23 Dianthrones of physcion
29
24 Heterodianthrone of chrysophanol and physcion 25 (R+) senno- side A 26 (mezo)sen- noside B 27 Aloesin 128 28 nepalenside A 128 29 nepalenside B 30 3-acetyl-2-methyl-1,5-dihydroxy-2,3- 134
epoxynaphthoquinols 31 3-Acetyl-2-methyl-1,4,5-trihy-droxy-2,3- 131
epoxynaphthoquinols 32 Nepodin 135; 94, 26 , 33 nepodin monoglucoside 42,136,121, 137, 34 patientoside A 138,128, 134 35 patientoside B Naphthalenes 36 Rumexoside 37 Orientaloside 38 Torachrysone 39 torachrysone-8-O-β-D-glucopyranoside 40 2-methoxystypandrone 136 41 Rumexneposide A 95 42 Rumexneposide 95 43 hastatuside B 135 44 Isovitexin 139
45 Apigenin 53
46 Vitexin 110, 139, 140
47 Luteolin 110
48 luteolin-7-O-glucoside 139, 126,53
49 Orientin Flavonoids 50 Isoorientin
30
51 Catechin 92, 141 52 Gallocatechin 142 53 6-chlorocatechin 92 54 catechin-6-C-glucoside 139 55 Epicatechin 28, 141, 142 56 Epigallocatechin
57 epicatechin-3-O-gallates 128, 142
58 epigallocatechin-3-O-gallates 59 procyanidin A2 143
60 (2R,2’R,3R,3’S,4R)- procyanidins B1 142, 143
61 (2R,2’R,3R,3’R,4R)-procyanidins B2
62 (2R,2’R,3S,3’S,4S)-procyanidins B3
63 (2R,2’R,3S,3’R,4S)- procyanidinsB4
64 (2R,2’R,3R,3’R,4S)- procyanidinsB5 143
65 (2R,2’R,3R,3’S,4S)- procyanidins B7
66 B2-3,3′ -O-digallate 142 67 epiafzelechin-(4β -8)-epicatechin 142 68 trans-resveratrol 28,144, 29 69 Pinostilbene
70 deoxyrhapontigenin 71 4-{(E)-2-(3,5-dihydroxyphenyl)ethenyl}-
1,2-benzenediols 72 4-{(E)-2-(3,5- Stilbenoids dihydroxyphenyl)ethenyl}phenyl-
hexopyranosides 73 4-[(E)-2-(3,5-dihydroxyphenyl)ethenyl]-2-
hydroxyphenyl-hexopyranosides 74 Piceid 75 (2-methoxy-2,4-dihydroxyphenol)-1-O-β- 128 Tannins
31
D-(6-O-galloyl)glucose 76 (3,5-dimethoxy-4-hydroxyphenol)-1-O-β- 143 D-(6-O-galloyl)glucose
77 2α,3α,19α-trihydroxys-24-norurs-4(23),12- 33
dien-28-oicacids
78 23-epoxy-2α,3α,19α-trihydroxys-24-norurs- 33 Triterpenes
12-en-28-oicacids 79 tormentic acid 33 80 myrianthic acid 33 81 Lutein 90,145 82 Anhydrolutein I 145 Carotenoids 83 Anhydrolutein II 145 84 β-carotene 90 85 Orcinol 92 86 2-acetylorcinol 26 87 Sakakin 128 , 26 88 2-acetylorcinol-3-O-glucoside 89 Rumexin 146 90 paraben-acid 131 91 vanillic acid 147 92 2,6-dihydroxybenzoic acid 131 Other 93 2,6-dimethoxy-4-hydroxybenzoic acid compounds 94 caffeic acid 146 95 1-methylcaffeic acid 148,147 96 1-O-caffeoyl-β-D-glucopyranoside 97 sinapic acid 98 Neochlorogenic acid 149 99 Hastatuside A 95 100 Lyoniresinol glucoside 128
32
2.4.1. Structures of the compounds
OH O OH OH O OH
HO 2 1 O O
OH O OH OH O OH
O 3 4 O O OH
OH O OH OH O OH
OH
HO 5 6 O OH O O
OH O OH O OH O OH
OH OH
HO O O 7 8 HO O O
HO
33
O OH glc O O OH
10 HO OH O 9 O
OH O OH OH O OH
OH O 11 12 OH O glc
O OH OH OH O OH O OH
10 13 14 OH OH O glc
OH O OH OH O OH O O OH OH
10 10 HO
16 OH 15 OH glc glc
34
OH O OH OH O OH O OH
10 10 HO HO 18 17 OH OH glc glc
OH O OH OH O OH
10 10 HO O 19 OH 20 OH glc glc
OH O OH OH O OH
10 O 10 21 OH glc 22
OH O OH
10 OH O OH O 23 O
OH O OH
35
OH O OH Oglc O OH
O 10 10 24 OH O 25 OH
OH O OH O glc O OH
Oglc O OH
O glc O 10 HO O O OH 26 OH 27
OH O
O glc O OH
O glc O OH O glc O OH OH O
HO HO HO O 28 HO O 29
36
OH OH
O O
O O 30 31 OH O OH OH
OH OH O glc O OH O
32 33 glc glc O OH O OH O
Cl
35 34 Cl Cl glc glc
O OH O glc O OH O
COOH 36 37
37
glc O OH O OH OH O
O O 39 38 O
O O O OH O O OH O
OH HO
HO
O 40 O 41 O
O O
O O O O O OH O O OH O OH HO OH HO HO HO
O 42 43
38
OH OH
HO O HO O
glc 44 45
OH O OH O
OH OH glc
HO O HO O OH
47 46 OH O OH O OH OH glc glc
HO O O O OH OH
49 48
OH O OH O
OH
HO O OH
glc 50
OH O
39
OH
OH OH
HO O HO O OH OH
OH OH 52 51 OH OH
OH OH
HO O HO O OH OH
OH glc OH Cl 54 53 OH OH OH
OH OH
HO O HO O OH OH
OH OH 56 55 OH OH OH
OH HO O OH
OH O
57 OH O OH
40
OH OH
HO OH OH
OH HO O OH OH O O OH
58 OH O OH OH OH OH O HO O OH 59 O OH OH OH OH OH OH O HO OH OH
OH OH O OH 60,61,62,63 OH OH OH O OH OH
OH 65 OH OH
OH OH HO O OH
OH OH HO O OH
OH 64 OH O OH
OH OH OH OH OH HO O OH
O 66 OH OH O
41
OH
OH OH O
HO
OH OH 68 OH OH HO O
OH
OH 67 OH O
OH HO
O 70 69
OH
OH Oglc
OH HO
HO OH 72
71 OH
OH OH Oglc glcO
HO OH 74
73 OH
OH
42
O O
O HO O O O O
O O HO HO O O O OH HO H HO O OH HO OH HO OH HO O 76 75
HO HO
COOH COOH HO HO
HO 78 HO 77 O
HO HO
COOH COOH HO HO
HO 80 HO 79 HO OH
81
HO
82
HO
43
83
HO
84
HO
O O
HO OH Oglc HO OH HO HO Oglc
86 85 87 88
O COOH COOH COOH
HO OH
OH O 90 89 91 92 Oglc OH OH OH
COOH O O
O O HO HO OH O
94 95 HO HO 93 OH
O O
O HO Oglc OH
96 97 HO HO
O
44
HO COOH
O HO O O
O OH
98 OH HO 99 Oglc OH
O OH O OH
Oglc HO
O 100 HO OH 101 O
O O
OH
45
2.5. R. Obtusifolius
Rumex obtusifolius (Polygonaceae) has long been used in traditional medicines. It is used as an depurative, astringent, antidote to nettle, laxative and tonic. It is also used to treat sores, tumors, blisters, cancer and burns [150].
This plant is very important in research point of view because of its traditional uses in medicine in several countries of South America. According to folk medicine this plant’s root has a prominent detoxifying result on the liver and is used against fever, jaundice, and as an anti- anemic tonic. The roots are also laxative. In addition, the leaves of this Rumex are used against hepatic, dermatological and eye problems. They are functional in the relief of furuncles, bruises and are also used as antiseptic and as scar healer [151].
Among the isolated compounds from this plant previously, we can find a glycopyranoside: 6-O- malonyl-β methylglucopyranoside [152]. Another effort has precise direction of the isolation and identification of amino acid plastocyanin [153]. Compound 101 (An anthraquinone) was isolated from R. Obtusifolius by Sandra L. etal in 2099 [154]. Compounds 4, 60, 61, 62, 65 have also been isolated from R. Obtusifolius [155, 127].
46
2.6. Biosynthesis of anthraquinones
In plants, anthraquinones are found in many species, especially in the plant families
Rhamnaceae, Polygonaceae, and Rubiaceae [156].
Anthraquinones are structurally made from an anthracene ring (tricyclic aromatic) with a keto group each on carbon atom nine and ten. In plants, two main biosynthetic pathways for the biosynthesis of anthraquinones have been described:
I. The shikimate or chorismate/o-succinylbenzoic acid pathway is used to synthesize
anthraquinones with only one hydroxylated ring like 1,2-dihydroxylated anthraquinone
(alizarin)
II. the polyketide pathway producing anthraquinones by folding of a polyketide chain with
both rings hydroxylated(emodin)[156, 157 and references therein]
Anthraquinones and their precursors, the anthrones, are widespread substances in many different organisms ranging from fungi, bacteria, plants and some animals [158, 159, 156].
47
O O O CO2 O
O O O HO SCoA SCoA 2 1 SCoA O O O 3
O R1
R8 R2
CO2
R7 R3
R6 O R4 4
Polyketide pathway for anthraquinone biosynthesis; 1 acetyl-CoA, 2 malonyl-CoA, 3 octa-â-ketoacyl chain, 4 Basic structure of Anthraquinone
OH O OH
HO
O
Emodin(1,8-dihydroxylated anthraquinone) from polyketide pathway
Scheme 2.1 Polyketide pathway for anthraquinone biosynthesis
48
HO COOH COOH COOH COOH O
HO A B C COOH OH O
COOH O R1 OH
R2
OH
D E OH O R3 OH
Shikimate pathway for anthraquinone biosynthesis; A shikimic acid, B o-succinoylbenzoic acid, 6 á- ketoglutaric acid,C mevalonic acid, D anthraquinone.
O OH
OH
O Alizarin(1,2-dihydroxylated anthraquinone) from shikimate pathway
Scheme 2.2 Shikimate pathway for anthraquinone biosynthesis
49
Chapter No 3
Result and Discussion
50
3.1. Preliminary phytochemical screeninig (qualitative) of crude extracts of R.Obtusifolius
The preliminary phytochemical analysis (qualitative) of the various extracts of R.Obtusifolius was done to evaluate the existence of bioactive components. The presence of alkaloids
(Dragendroff, Wagner, Mayer), tannins, flavonoids, anthraquinones, steroids, cardiac glycosides and saponins was analyzed (Table 3.1).
Results of different experiments performed for phytochemical screening revealed that alkaloids are absent in n-hexane and aqueous extracts. Alkaloids are present in lower amount (+) with
Dragondroff test and Wagner test in DCM extract, while considerable amount is present with
Wagner test in ethyl acetate extract. Tannins are only present in considerable amount in DCM and ethyl acetate extracts. Cardiac glycosides and Steroids are present in all extracts except n- hexane. DCM and ethyl acetate extracts contain considerable amount of Anthraquinones. The table 3.1 results show that flavonoids are present in all the tested extracts.
51
Table 3.1. Preliminary qualitative phytochemical analysis of crude extracts of R.Obtusifolius
Alkaloids S.No Extracts TN CG ST FL SP AN DR MR WR
1 n-hexane ------+ - -
2 DCM + - + ++ + ++ ++ + ++
3 Ethyl acetate + + ++ ++ +++ ++ ++ +++ ++
4 Aqueous - - - - + + + - -
MR= Mayer’s reagent; DR= Dragondroff’s reagent; WR= Wagner’s reagent; TN=Tannins;
FL=Flavonoids; ST=Steroids; SP=Saponins; CG=Cardiac glycosides; AN=Anthraquinones and -
= Absent; + = present; ++= present considerable; +++ = present very considerable.
52
3.2. Biological Screening of Dichloromethane Sub fractions of Rumex Obtusifolius
3.2.1. Antibacterial screening
A disc diffusion method was performed to assess the antibacterial screening of sub-fractions of
Dichloromethane fraction of Rumex obtusifolius. The results are presented in table No 3.2. The
F1 and F2 do not show any antibacterial property. The F6 is active against all bacteria, while F3 is active only against E. coli. The most significant antibacterial properties are seen for F6. Highest zone of inhibition (22.5 mm) is showed for F6 against Ampicillin-resistant Escherichia coli.
Table No 3.2 shows that generally activity increases with polarity. The antibacterial effects of
DCM fraction of Rumex obtusifolius is mostly due to average polarity compounds, e.g.
(flavonoids, phenolics) present in medium polar fractions F4, F5 and F6. It is also cleared that the active compounds accountable for antibacterial effects is more soluble in polar organic solvent.
Antibacterial screening of all the six fractions is also shown in figure No 3.1.
53
Table No3.2. Antibacterial activities of the sub- fractions of DCM fraction of R. obtusifolius (in mm)
Sub-fractions 1 2 3 4 5 6 7 8
F1 R R r r r R r R
F2 R R r r r R r R
F3 R R r r r R r R
F4 13 9 14 19 8 12.5 9.5 R
F5 14 11 17.5 11 9 13 10.5 R
F6 15 14 16 22.5 9 14.5 11 10
Cefotaxime 32 31 30 30 30 30 30.5 30
̽1 = Bacillus cereuss , 2 = Bacillus subtilis , 3 = Escherichia coli , 4 = Ampicillin-resistant
Escherichia coli , 5 = Staphylococcus aureuss and 6 = Salmonella typhii , 7= Pseudomonas
aeruginosas ,8= Streptococcus pneumonia. r=Resistant=Show no activity
54
3.2.2. Antifungal screening
The results of table No 3.3 indicate that F3, F4 and F5 inhibited fungal growth more proficiently as compared to F1, F2 and F6. Maximum inhibition was recorded by F4 is 69.4% against Aspergillus flavas. F4 and F5 show significant inhibition ranging (35.1±2.21 to 69.4±3.18) except F4 against
Fusarium moniliformes.F1does not show any prominent antifungal activity (7.4±2.51 to10.3±2.21) against all fungi, b/c the probability of bioactive agents in F1 is less, as ethanolic crude was already extracted with n-haxane in solvent extraction procedure. Shortly, F4 is the most active and F1 least active among the 6 fractions. The results confirm previous study in which fungi toxic surface flavonoids (Isoflavonoid) have been isolated and characterized are reported to be extracted with low polar solvents and non polar [160], like n-hexane and DCM mixture. Percentage inhibition of fungi has been shown in figure No 3.1.
55
Table 3.3. % Inhibition of fungi of DCM sub-fractions of R. obtusifolius
Fractions A.flavass F.solani M.species A.nigers A.fumigatus A.alterata F.moniliformes
F1 9.4±1.39 10.3±2.1 8.2±1.4 9.4±2.85 8.4 ± 2.53 9.8±1.39 7.4 ± 2.51
F2 30.2±1.3 15.3±1.3 23.6±1.32 14.2±2.1 21.3±1.43 37.4±2.2 23.8±2.13
F3 25.4±2.53 15.8±1.39 14.1 ± 1.51 31.7±2.49 31.7 ± 2.49 31.7±2.49 34.2±1.25
F4 69.4±3.18 36.4±1.89 38.0 ± 1.34 36.0±1.68 56.2 ± 2.77 37.6±1.32 30.1±1.31
F5 66.2±1.41 36.2±2.14 41.3±1.34 49.1±1.23 50.2±2.41 42.4±2.51 35.1±2.21
F6 22.6±2.32 27.0±2.56 43.2 ± 1.80 51.3±1.67 15.5 ± 2.34 40.5±1.07 30.4±1.34
Terbinafin 87.6±2.70 84.5±2.13 81.78±2.12 88.4±3.16 87.4 ± 3.17 84.4±3.13 89.2±1.23
DMSO N N N N N N N
Mean ± SE and N = Nil
56
100%
90%
80%
70%
60% Terbinafin F6 50% F5
40% F4 F3 30% F2 F1 20%
10%
0%
Fig 3.1. percentage inhibition of fungi of DCM sub-fractions of R. obtusifolius
57
3.2.3. Cytotoxicity screening
Brine shrimp assay is recommended to be a suitable tool for the pharmacological activities in plant analysis [161]. Cytotoxicity results are presented in Table No 3.4. The results indicate that the F4 is the most active (LD50 437.4), having maximum mortality of brine shrimp (66.65%) at
100ppm, while F1 is the least active fraction. Our results showed that none of the fractions are found highly effective (P > 0.05), however at high concentration, fractions were effective at probability level 0.05. Other fractions do not any show prominent results, as higher the value of
LD50 lower will be percentage mortality of brine shrimp. It can be thought that presence of a wide range of bioactive compounds with different structures and their synergistic effect may put in to the overall activity of F4. F1, F2, F4 has shown lowest % mortality of brine shrimp at 10 ppm, while it has highest value at 1000 ppm (66.6%). Figure No 3.2 Illustrated percentage mortality of brine shrimps at different concentrations of sub-fractions, while respective LD50 values of brine shrimps at different concentrations have been shown in figure No 3.3.
58
Table 3.4. Illustration of percentage mortality of brine shrimps at different concentrations of sub-fractions and respective LD50 values
Concentration F1 F2 F3 F4 F5 F6
10ppm 13.3 % 23.3% 13.3 % 13.3 % 20.0 % 16.6%
100ppm 23.3% 30.0% 16.6% 20.0% 26.6% 20.0%
1000ppm 30.0% 43.3% 56.6% 66.6% 50.0% 50.0%
LD50 values 53970.9 4753.8 867.8 437.4 1371.8 1552.1
59
70.00%
60.00%
50.00%
40.00% 10ppm 100ppm 30.00% 1000ppm
20.00%
10.00%
0.00% F1 F2 F3 F4 F5 F6
Fig No: 3.2. Illustration of percentage mortality of brine shrimps at different concentrations of sub-fractions.
60
60000
50000
40000
30000 LD50 values
20000
10000
0 F1 F2 F3 F4 F5 F6
Fig 3.3. Illustration of respective LD50 values of brine shrimps at different concentrations of sub-fractions
61
3.3. Secondary metabolites from Rumex Obtusifolius
In search of bioactive secondary metabolites from medicinal plants, Rumex Obtusifolius belonging to the genus rumex was investigated. The ethno-pharmacological and chemotaxonomic importance of the genus prompts us to start evaluation and screening on this plant. As a result, four compounds were isolated from DCM soluble fraction of Rumex
Obtusifolius. (Scheme -1, 2)
Structures of the all isolated compounds were elucidated using spectral as well as published data in literature. In this section of my project, the compounds are discussed briefly.
3.4. DCM soluble fraction
The DCM soluble fraction was concentrated and subjected to column chromatography over silica gel for preliminary fractionation. Elution was carried out with n-hexane 100 % (F1), n- hexane75% - DCM 25% ( F2), n-hexane 50% - DCM50% (F3), n-hexane25% - DCM75%(F4),
DCM100%(F5), EtOAc100%(F6), in increasing order of polarities.
It has been that F4, F5 and F6 sub-fractions of DCM fraction of Rumex obtusifolius appeared as an important source for the discovery of new cytotoxic, antibacterial and antifungal agents in biological screening, therefore these fractions were further loaded to a series of column chromatography to obtain four anthraquinone compounds, Obtusifolate A(102), Obtusifolate
B(103), Obtusifolate C(104) and Obtusifolate D(105).
All the compounds were characterized using latest spectroscopic techniques and chemical methods.
62
3.5. Structure elucidation of compounds.
3.5.1. Obtusifolate A (102)
19 O OH O OH
21 18 17 1 9a 9 8a 8 O 13 6' 3 6 4a 10 10a 16 1' 5 12
4' 2' O 11 14 1'' 4'' H 5'' 2'' O 3'' Obtusifolate A (102) O 7'' 6'' 8''
The fraction F4 obtained with n-hexane - DCM (25%: 75%) was subjected to column chromatography over silica gel eluting with n-hexane – DCM mixtures in increasing order of polarities. The compound obtained as yellow amorphous solid from n-hexane - DCM (1:9) was identified as Obtusifolate A (102). The Compound was elucidated through UV-VISIBLE, IR,
NMR and MS studies as an anthraquinone derivate.
3.5.1.1. UV-Visible and IR of Obtusifolate A (102)
The absorptions at (3441,3425), (1701–1728), (1590) and (1619) in cm-1 of the IR spectrum showed the presence of chelated hydroxyl groups, ester groups, conjugated carbonyl groups of anthraquinone nucleus and benzene ring respectively. Absorption at 1715 cm-1 is due to non
63
conjugated carbonyl group. The UV spectra of compound (102) showed maximum absorptions at
211, 239, 252, 275, and 366 nm, attributed a highly conjugated system [162].
3.5.1.2. Mass spectrometry of Obtusifolate A (102)
The molecular formula was determined through HREI-MS as C39H42O8 (m/z =638.2870; calcd.
638.2880), which shows 15 degrees of unsaturation. Eight of them are eventually accounted for anthraquinone ring, 3 for the tri-substituted benzene ring; one was due to double bonds, two for ketonic and last one for ester carbonyls group.
3.5.1.3. 1H-NMR spectrum of Obtusifolate A (102)
The 1H-NMR spectrum of compound (102) confirm alkene moiety (double bond) with a proton at (6.69ppm, s) together with two different methyl groups at (1.65ppm, s), (1.70ppm, s) attached to the same double bonded carbon. Two singlet’s at (12.13ppm, HO-1) and (12.31ppm, HO-8) revealed the presence of two peri-positioned chelated hydroxyl groups [163, 164].
Two peri-positioned chelated hydroxyl groups together with two conjugated carbonyl groups(C-
9, δ190.50; C-10; δ181.00)ppm confirmed the presence of anthraquinone nucleus. A pair of singlet appearing at (7.02ppm, H-4) and (7.12ppm, H-7) indicated a tetra-substituted 1,8- dihydroxy anthraquinone. A mutiplet at 4.20ppm corresponding to H-18 was attributed to the oxymethylene protons. Signals at (7.66d, H-3') due to meta coupling having small J (3Hz) value;
(7.72dd, H-5' J=3&8.8Hz) corresponding to ortho and meta coupling; (7.56d, H-6' J=8.8) for ortho coupling) showing another benzene ring. Signals at (2.38s, H-11 &2.13s, H-3'') having same height indicated methyl groups directly attached to aromatic ring and to carbonyl group respectively. A singlet at (3.62ppm, H-1'') was due to methylene group present b/w carbonyl and aromatic ring. A highest singlet in up field region (1.28s, H-13 and H-14) confirmed two methyl
64
groups in same chemically environment. The up field signals (0.85—1.70ppm) were due to protons of various chains of alkyl groups listed in table No 3.5.
3.5.1.4. 13C NMR spectrum of Obtusifolate A (102)
13C NMR spectrum determined through a DEPT (Distortionless Enhancement by Polarization
Transfer) experiment shows 38 signals for 39 carbon atoms, in which 20 are for olefinic , four for carbonyl, and the remaining are for SP3 carbons of methane, methylene and methyl groups.
The most downfield signal at (206.01ppm) is assigned to non-conjugated carbonyl carbon. Other downfield signals at (190.50, 181.00)ppm and (168.12)ppm are assigned to the conjugated carbonyls of anthraquinone ring and ester carbonyl respectively. The enone portion C=O resonated at (192.10ppm, C-4''). The carbon signal appearing at 74.00ppm is attributed to the oxymethine carbon. The most important signals, which appears at (165.42, 159.00)ppm are assigned for C-1 and C-8 to which chelated hydroxyl groups are attached. Another up field signal at 29.60ppm is due to C-13 and C-14, which confirmed two methyl groups carbons in almost same chemically environment (table No 3.5).
3.5.1.5. Other chemical tests for identification Obtusifolate A (102)
Compound (102) decolorized KMnO4 solution, which showed non-aromatic multiple bonds
(double or triple bond).
The stereochemistry at the chiral center C-18 was determined by the alkaline hydrolysis of A that yielded an alcohol that could be identified as (R)-1-methyl-1-propanol through the sign of its optical rotation.
65
Table No 3.5 1HNMR and 13CNMR data of Obtusifolate A(102) (δ=chemical shift in ppm) Obtusifolate A (102) Position δ (H) δ(C) 1-OH 12.31 165.42 2 ---- 117.00 3 ---- 138.90 4 7.02s 124.50 5 ---- 144.00 6 ---- 150.13 7 7.12s 144.40 8-OH 12.13s 159.00 9, ----- 190.50, 10 ----- 181.00 4a ----- 134.04 8a ----- 114.20 9a ----- 113.10 10a ----- 133.15 11 2.38s 20.01 12 ---- 34.50 13 1.28s 29.60 14 1.28s 29.60 15 1.20q 37.6 16 0.85d 9.00 17 ----- 168.12 18 4.20m 74.00 19 1.35d 22.02 20 1.75m 29.80 21 0.92 t 8.01 1' ----- 138.70 2' ----- 132.30 3' 7.66 d 129.40 4' ----- 136.60 5' 7.72 dd 127.80 6' 7.56d 127.50 1'' 3.62s 48.4 2'' ----- 206.01 3'' 2.13s 31.30 4'' ----- 192.10 5'' 6.69s 120.00 6'' ----- 133.10 7'' 1.65s 18.50 8'' 1.70s 25.50
66
3.5.2. Obtusifolate B (103)
O OH O OH 18 1 9a 9 8a 8 O 17 13 6' 3 6 10 10a 4a 16 1' 5 12 4' O 11 14 3' 7' 1'' Obtusifolate B (103) O 2'' 4'' H 3''
5''
The eluate obtained with 100% DCM of F4 showed one major with some minor spots on TLC were and re-chromatographed with mixtures of EtOAc - DCM in increasing polarities over silica gel. A fraction with EtOAc – DCM (1:9) contained the compound corresponding to the major spots. It was concentrated and was elucidated through UV-Visible, IR, NMR and MS studies as an anthraquinone derivate.
3.5.2.1. UV-Visible and IR of B (103)
The absorptions at (3441, 3425), (1701–1728), (1590) and (1619) in cm-1 of the IR spectrum showed the presence of chelated hydroxyl groups, ester groups, conjugated carbonyl groups of anthraquinone nucleus and benzene ring respectively.
The UV spectra of 103 showed maximum absorptions at 211, 252, 275, and 366 nm, attributed a highly conjugated system [162].
67
3.5.2.2. Mass spectrometry of B (103)
Through HREI-MS the molecular formula of compound 103 was determined as, C34H34O7 molecular ion peak (m/z =554.2296; calcd. 554.2305), which shows 14 degrees of unsaturation.
Eight of them are accounted for anthraquinone ring, 3 for the trisubstituted benzene ring; one was due to double bonds, one for ketonic and last one for ester carbonyls group.
3.5.2.3. 1HNMR spectrum of B (103)
The 1HNMR and 13CNMR of (103) is similar to compound (102) with little differences as shown in table No 3.5. Two singlets (12.14ppm, HO-1, and 12.33ppm, HO-8) revealed the presence of two peri-positioned chelated hydroxyl groups [163, 164]. Two peri-positioned chelated hydroxyl groups together with two conjugated carbonyl groups(C-9, 190.50ppm; C-10,181.00ppm) also confirmed the presence of anthraquinone nucleus in compound (103).
A pair of singlet appearing at (7.02, H-4) and (7.12, H-7) indicated a tetra-substituted 1,8- dihydroxy anthraquinone. A singlet at 4.23ppm corresponding to H-18 was attributed to the oxymethylene protons. Signals at {7.66d H-3' due to meta coupling having small J values; (7.72-
7.74 dd H-5') corresponding to ortho and meta coupling; (7.56d H-6') for ortho coupling} showing another benzene ring as in compound (103). Signals at (2.38s H-11 and 2.47s H-3'') having same height indicated Me groups directly attached to aromatic rings. A highest singlet in up field region (1.28ppm, H-13 &H-14) also confirmed two methyl groups in same chemically environment in compound (103). The up field signals (0.85—1.70ppm) were due to protons of various chains of alkyl groups listed in table 3.6.
68
3.5.2.4. 13C NMR spectrum of B (103)
The 13C NMR spectrum determined through a DEPT experiment shows 33 signals for 34 carbon atoms, in which 16 are for olefinic , three for carbonyl, and the remaining are for SP3 carbons of various methine, methylene and methyl groups. The most downfield signals at (190.50ppm,
181.00ppm) and (166.10ppm) are assigned to the conjugated carbonyls of anthraquinone ring and ester carbonyl respectively. The enone portion C=O resonated at (192.10, C-1''). The carbon signal appearing at (51.60ppm) is attributed to the oxymethyl carbon. The most important signals, which appears at (165.00, 159.00)ppm are assigned for C-1 and C-8 to which chelated hydroxyl groups are attached. Another up field signal at 29.60ppm is due to C-13 and C-14, which confirmed two methyl groups carbons in almost same chemically environment. The different olefinic carbons resonated at (113.00—150.00) which are present in various chemical environments are listed in table No 3.6.
3.5.2.5. Other chemical tests for identification Obtusifolate B (103)
Compound Obtusifolate B (103) also decolorized KMnO4 solution, which showed non-aromatic multiple bonds (double or triple bond).
69
Table No 3.6 1HNMR and 13CNMR data of Obtusifolate B(103), (δ=chemical shift in ppm) Obtusifolate B (103) Position δ (H) δ(C) 1-OH 12.33 165.00 2 ---- 116.01 3 ---- 138.60 4 7.02s 124.55 5 ---- 144.00 6 ---- 150.14 7 7.12s 144.40 8-OH 12.14 159.00 9 ----- 190.50 10 ----- 181.00 4a ------134.04 8a ----- 114.20 9a ----- 113.10 10a ----- 133.15 11 2.38s 20.00 12 ---- 34.50 13,14 1.28s 29.60 15 1.20q 37.6 16 0.85d 9.00 17 ---- 166.10 18 4.23s 51.60 1' ---- 139.50 2' ---- 136.70 3' 7.66 d 130.00 4' ---- 136.60 5' 7.72dd 127.80 6' 7.56d 127.50 7' 2.47s 22.50 1'' ---- 192.10 2'' 6.69s 120.00 3'' ---- 133.10 4'' 1.65s 18.50 5'' 1.70s 25.50
70
3.5.3. Obtusifolate C (104)
O 23 O 8 1 21 13 17 7 8a 9 1a O 11 18 20 12 19 O 3 5a 10 4a 5 4
O 14 O 15 Obtusifolate C(104)
16
F6 fraction was subjected to column chromatography over silica gel, eluting with n-hexane, n- hexane/DCM, DCM/AcOEt, AcOEt and MeOH in increasing order of polarity. Eluting with the solvent system AcOEt /DCM 2:1 to afford Obtusifolate C (104). It was then purified by pencil column chromatography and concentrated as an orange gummy solid.
3.5.3.1. UV and IR spectra of Obtusifolate C (104)
In UV spectra intense benzenoid absorption at 240-260 nm, medium absorption at 320-330 nm a strong quinonoid electron transfer band at 270-290nm accompanied by a weak quinonoid absorption band at 405 nm showed anthraquinones skeleton. The absorptions at (1701–1728) and
(1590) in cm-1 of the IR spectrum showed the presence of ester group and conjugated carbonyl groups of anthraquinone nucleus. Absorption at 1715cm-1 is due to non conjugated carbonyl group (C-15).
71
3.5.3.2. Mass spectrometry of Obtusifolate C (104)
The molecular formula was determined through HREI-MS as C27H28O6 (m/z=448.1876; calcd.
448.1886), which shows 11 degrees of unsaturation. Eight of them are eventually accounted for anthraquinone ring, two for ketonic and last one for ester carbonyls group.
3.5.3.3. 1HNMR spectrum of Obtusifolate C (104)
Two pair of doublets appearing at (7.55ppm, H-4, J=8Hz & 7.57ppm, H-3, J=8Hz) and
(7.72ppm, H-6, J=3Hz & 7.74ppm, H-8, J=3Hz) due ortho and meta coupling respectively indicated a tetra-substituted anthraquinone. Signals at (2.39s H-23 &2.13s H-16) having same height indicated methyl groups directly attached to aromatic ring and to carbonyl group respectively. A singlet at (3.91ppm, H-14) was due to methylene group present between carbonyl and anthraquinone ring. A highest singlet in up field region (1.35ppm, H-19 and H-20) confirmed two methyl groups in same chemically environment. The various up field signals at
(0.96-1.28) ppm were due to protons of various chains of alkyl groups listed in Table No 3.7.
3.5.3.4. 13C NMR spectrum of Obtusifolate C (104)
13C NMR spectrum shows 26 signals for 27 carbon atoms, in which 12 are for olefinic, four for carbonyl, one for ester and the remaining are for SP3 carbons of methine, methylene and methyl groups.
The most downfield signals at 209.00ppm and 206.01ppm are assigned to C-17 and C-15 carbonyl carbons. Other downfield peaks at (181.00, 182.50) ppm and (168.12) ppm are assigned to the carbonyls carbons of anthraquinone ring and ester carbonyl carbon respectively.
72
The signal at 72.50ppm is attributed to the oxy-methylene carbon. Another up field signal at
22.02ppm assigned to C-19 and C-20 confirmed two methyl groups carbons in almost same chemically environment. All the above evidences confirmed the structure of compound (104).
(table No 3.7).
3.5.3.5. Other chemical tests for identification Obtusifolate C (104)
It gave red solutions on reduction in alkaline solution (in aqueous sodium hydroxide, which distinguished anthraquinone from benzoquinones and naphthoquinones [165].
73
Table No 3.7 1HNMR and 13CNMR data of Obtusifolate C (δ=chemical shift in ppm) Obtusifolate C (104) Position δ (H) δ(C) 1 ------144.00 2 ------136.60 3 7.57d 127.80 4 7.55d 127.50 5 ---- 132.30 6 7.72d 129.40 7 ----- 117.00 8 7.74d 124.50 9 ------181.00 10 ------182.50 1a ------134.04 8a ------133.15 4a ------132.00 5a ------132.50 11 ------168.12 12 4.23q 72.50 13 1.28t 22.70 14 3.91s 48.40 15 ---- 206.01 16 2.13s 31.30 17 ------209.00 18 ----- 48.40 19 1.35s 22.02 20 1.35s 22.02 21 1.42q 34.50 22 0.93t 9.00 23 2.39s 20.01
74
3.5.4. Obtusifolate D (105)
O 21 O 8 1 19 13 8a 9 1a O 15 11 7 16 18 12 17 O 3 5a 10 4a 5 4 Obtusifolate D (105) 14 O O
F6 fraction was subjected to column chromatography over silica gel, eluting with n-hexane, n- hexane/DCM, DCM/AcOEt, AcOEt and MeOH in increasing order of polarity. Eluting with the solvent system AcOEt /DCM 1:1 Obtusifolate D (105) was obtained as an orange gummy solid.
3.5.4.1. UV and IR spectra of Obtusifolate D
The UV spectra confirm anthraquinones skeleton as in compound (104). The absorptions at
(1701–1728) and (1590) in cm-1 of the IR spectrum showed the presence of ester group and conjugated carbonyl groups of anthraquinone nucleus but a peak at 1715 cm-1 was found to be disappear which showed the absence of non conjugated carbonyl group in compound (105). An additional strong absorption at 1270--1230 cm-1 showed the ether functionality.
3.5.4.2. Mass spectrometry of Obtusifolate D (105)
The molecular formula was determined by HREI-MS as C25H26O6 (m/z =422.1719; calcd.
422.1729), which shows 10 degrees of unsaturation. Eight of them are eventually accounted for anthraquinone ring, one for ketonic and last one for ester carbonyls group.
75
3.5.4.3. 1H-NMR and 13C-NMR spectra of compound D (105)
The1H-NMR and 13C-NMR spectra of compound (105) (Table 3.8) was very similar to that of
(104), except for the presence of additional peaks due to ether group (H-14, 3.79s, 56.60=C-14) plus absence of carbonyl group peaks (H-14=3.91s, H-16=2.13s, C-14=48.40, C-15=206.01,C-
16=31.30) in ppm of compound (104). 1H-NMR and 13C-NMR spectra and molecular formula determined by HREI-MS showed that CH3O- group is present in compound (105) in place –CH2-
CO-CH3 group of compound (104).
3.5.4.4. Other chemical tests for identification of Obtusifolate D (105)
It also gave red solutions on reduction in alkaline solution (in aqueous sodium hydroxide, which distinguished anthraquinone from benzoquinones and naphthoquinones [165].
76
Table No 3.8 1HNMR and 13CNMR data of Obtusifolate D (δ=chemical shift in ppm) Obtusifolate D (105) Position δ (H) δ(C) 1 ------144.00 2 ------136.60 3 7.57d 127.80 4 7.55d 127.50 5 ---- 150.13 6 7.72d 129.40 7 ----- 117.00 8 7.74d 124.50 9 ------181.00 10 ------182.50 1a ------134.04 8a ------133.15 4a ------132.00 5a ------132.50 11 ------168.12 12 4.23q 72.50 13 1.28t 22.70 14 3.79s 56.60 15 ------209.00 16 ----- 48.40 17 1.35s 22.02 18 1.35s 22.02 18 1.42q 34.50 20 0.93t 9.00 21 2.39s 20.01
77
3.6. Free radical scavenging activity of the isolated compounds
The results of table No 3.9 show prominent radical scavenging activity for 102 & 103. There is a very little difference in RSA b/w the two compounds. Both of the compounds have greater radical scavenging property than ascorbic and gallic acid.
The results indicate significant radical scavenging activity for 104 & 105. Both the compounds have round about same RSA. Both of the isolated compounds have less radical scavenging property than ascorbic and gallic acid. %DPPH inhibition has been shown graphically for all the four isolated compounds (fig 3.1).
Table 3.9 Percentage of RSA of compounds 102, 103, 104 and 105 from Rumex Obtusifolius
S.No Compounds/standards % DPPH inhibition±SEM 1 A 97.55±1.51 2 B 96.00±0.83 3 Gallic acid 93.00±0.29 4 Ascorbic acid 92.33±0.55 5 C 80.12±0.91 6 D 79.00±1.17
78
Fig 3.4 % DPPH inhibibition zone of compound the four isolated compounds from Rumex obtusifolius
% DPPH inhibition±SEM 120
100
80
60
40
20
0 A B Gallic acid Ascorbic C D acid
79
Chapter No 4
Experimental
80
4.1. Plant collection, Identification and Grinding
The whole plant except fruit and seed of Rumex obtusifolius (Polygonaceae) was collected from
Bannu, KPK, Pakistan at December 2015 and identified by Prof. Abdur Rehman, Botany
Department, GPG College Bannu. The plant was washed, shade dried and was then grinded into powders using electrical grinder.
4.2. Extraction and Fractionations
The powders of the grinded plant were extracted with ethanol for 14 days at room temperature.
Ethanolic extract was evaporated by rotary to obtain gummy crude. The crude was successively fractionated with increasing order of polarity i.e. n-hexane, dichloromethane, ethylacetate and ethanol by separating funnel as shown in scheme 1.
4.3. Preliminary qualitative phytochemical analysis [166, 167].
4.3.1. Alkaloids
Each extract was evaporated in a boiling water bath and the residue was mixed with 2N HCl.
Then the mixture was filtered. The filtrate was divided into three equal parts. One part was mixed with a few drops of Mayer's reagent; one portion was treated with equal amount of
Wagner's reagent and the other portion was reacted with equal amount of Dragondroff’s reagent.
The creamish, brown and orange precipitate indicated the presence of respective alkaloids [168].
4.3.2. Flavonoids
The existence of flavonoids was analyzed by Shinoda experiment. Each extract was reacted with a few drops of concentrated Hydrochloric acid and Mg- ribbon. The appearance of tomato red or pink colour within a few minutes confirmed the presence of flavonoids [169].
81
4.3.3. Tannins
Each extract dry powder form was treated with alcoholic FeCl3 reagent. Appearance of blue color indicated the presence of tannins [170].
4.3.4. Cardiac glycosides
Keller-kiliani experiment was carried out to judge the existence of cardiac glycosides. The crude
3 dry powder of each extract was mixed with 1cm of FeCl3 reagent (mixture of 1 part of 5 percent
FeCl3 solution and 99 part of glacial acetic acid). To this solution a few drops of concentrated
H2SO4 was added. Greenish blue color within a few minutes indicated that cardiac glycosides was present [171].
4.3.5. Anthraquinones
About 500mg of each extract was mixed with 10% HCl and boiled on water bath. It then filtered and filtrate was allowed to cool. Equal volume of chloroform was added the filtrate and then few drops of 10% NH3 was added to mixture and heated. The appearance of Rose-pink color indicates the presence of anthraquinones.
4.3.6. Steroids
Liebermann-Burchard test was conducted to evaluate the presence of steroids. A chloroform solution of the crude dry powder of each extract was treated with acetic anhydride and a few drops of concentrated H2SO4 were added. The appearance of blue green ring indicated the presence of steroids.
82
4.3.7. Saponins
The existence of saponins was tested by Frothing procedure. The crude dry powder of each extract was vigorously shaken with distilled water and was allowed to stand for ten minutes. No froth indicates absence of saponins while stable froth more than 1.5 cm indicated that saponins are present [172].
4.4. Sub-fractionation of Dichloromethane soluble fraction
Dichloromethane (DCM) fraction was Sub-fractionated into several fractions (F1, F2, F3, F4, F5 and F6) using column chromatography as presented in table No 4.1. All the fractions were evaporated by rotary evaporator. These fractions were screened for biological activities.
83
Table No 4.1 Sub-fractionation of Dichloromethane soluble fraction
Sub- Eluents fractions
% DCM %n-hexane
F1 0 100
F2 25 75
F3 50 50
F4 75 25
F5 100 0
F6 100% ethyl acetate was eluted at the end.
84
4.5. Biological Screening of Dichloromethane Sub-fractions of R. obtusifolius
4.5.1. Antibacterial screening
Test bacteria: Antibacterial screening of different fractions was performed for eight pathogenic
bacteria i.e. Bacillussubtiliss (NCTC 10400), Escherichia coli (ATCC 8739), ampicillin-resistant
Escherichia coli (NCTC 10418), Bacillus cereus (ATCC 11778), Staphylococcus aureuss (NCTC
1803), Pseudomonas aeruginosas (ATCC 27853), Streptococcus pneumonia (ATCC 49619),
Salmonella typhii (NCTC 10203), obtained from Biotechnology Department of UST Bannu,
Pakistan.
Procedure: The antibacterial assay was performed by a common disc diffusion process [173,
174]. Briefly, the concentration was 500 × 10-6 g/disc in case of each extract. The sample discs and positive controls (cefotaxime, 10 × 10-6 g/disc) along with negative control discs were placed on Petri dishes having suitable agar medium seeded with the test microorganisms using sterile
transfer loop and kept at 4 °C to assist maximum diffusion s. All the plates were incubated at 37
°C for bacterial growth. The diameter of clear area in the Petri dish which was devoid of bacterial growth was calculated which showed antibacterial activity of the test agents in terms of mm.
4.5.2. Antifungal screening
Test fungi: , Aspergillus flavass, Fusarium solanii, Aspergillus nigers, Mueor species, Fusarium moniliformes, Alternaria alterata, Aspergillus fumigates.
Procedure: An agar tube dilution method was conducted for antifungal screening of the factions was investigated according to the procedure reported by Choudhary et al [175]. Briefly, to
3 prepare media for fungi 32.5 g savored dextrose agar was mixed with 500 cm distill H2O. Then it was heated to be dissolved and 5 cm3 was dispensed into screw cap tubes. The tubes were
85
marked and autoclaved at 121°C for 20 minutes. All the tubes were then allowed to cool. 100 ×
10-6 L of extract (0.02 g/cm3 in DMSO) and 83 × 10-6 L of terbinafine (0.012 g/cm3 in DMSO) were mixed just before solidification, as positive control in tubes to get concentration of 0.4 and
0.2 × 10-3 g/cm3, respectively. Add 0.1 mg per tube DMSO was used as negative control. Each tube was inoculated with a 4 mm diameter piece of inoculum from a culture seven days. All these tubes were incubated at 27 °C for 7 days. Fungal growth was calculated by measuring linear growth in terms of mm. % inhibition of fungal growth was finalized by the following equation.
A X = [100 − ] × 100 B
Where; A= linear growth in test (mm), B= linear growth in control (mm), X= Percentage inhibition of fungal growth.
4.5.3. Cytotoxic screening
Cytotoxic activity for DCM sub- fractions were analyzed by performing brine shrimps hatched in saline process, as reported by Meyer-Alber et al. [176], with slight modification. Briefly, 20 mg each sample was dissolved in 2cm3 of respective solvent. From this stock solution 5 × 10-6 L, 50
×10-6 L and 500 × 10-6 L was poured separately into 5mL; 20mL 50 mL vials respectively. They were placed open in continuous air flow for dryness. 3 cm3 artificial sea water was added in each vial and then 10 matured brine shrimp larvae were also added. At last sea water was poured up to the mark and 10, 100, 1000 ppm working solution were prepared by simple dilution method.
They were kept under illumination and after 24h of incubation survivors were counted by magnifying glass. LD50 value was calculated by probit analysis in finny computer software.
86
4.6. Secondary metabolites from R. Obtusifolius
As fractions (F1, F2, F3, F4, F5 and F6) have been screened for biological activities, in which F4,
F5 and F6 were proved to be the most active antibacterial, cytotoxic and antifungal agents [177], so they were further subjected to column chromatography to isolate various secondary metabolites.
4.6.1. Instrumentation
Melting points were measured by using Gallenkamp and Kofler hot-stage apparatus. Glass capillaries were used and melting points are uncorrected. All the solvents were distilled before use .1H-NMR and 13C-NMR spectra were recorded with a Brucker spectrometer operating at 500
MHz and 100 MHz respectively, using CDCl3 (δH 7.26, δC 77.00 ppm) as a solvent. Chemical shift values are reported relative to TMS. The Mass spectra (MS) were determined using
Micromаss ZMD and Varian MAT 312 double focusing mass spectrometer coupled to DEC–
PDP 11 / 34 computer system. Shimadzu 460 and Shimadzu UV-2401PC spectrometers were used for IR and UV spectra determination respectively.
4.6.2. Chromatography
Silica gel (230–400 mesh) for column chromatography and aluminum sheets coated with silica gel 60F245 (20cm × 20 cm) 0.2mm thick; were used for TLC (E.Merck).Visualization of the spots on TLC plates was carried out by UV at 254 and 366 nm.
87
4.6.3. Isolation, Purification and Characterization of compounds
F5 fraction was subjected to column chromatography over silica gel, eluting with increasing polarity n-hexane, n-hexane/DCM, DCM /AcOEt, and MeOH. Eluting with the solvent system n- hexane/DCM (1:9) to afford compound 102 while compound 103 was obtained in semi-pure form from the column by using DCM/AcOEt (9:1) as eluent. It was purified by pencil column chromatography.
Fraction (F6) was also subjected to column chromatography over silica gel, eluting with n- hexane, n-hexane/DCM, DCM/AcOEt, AcOEt and MeOH in increasing order of polarity.
Eluting with the solvent system AcOEt /DCM 1:1 to afford comound105 and 104 was obtained in semi-pure form from the column by using DCM/AcOEt 1:2 as eluent as given in scheme 2.
88
R. obtusifolius 15 Kg
Ethanolic Extract (Crude) 780g
Extracted with n-hexane Water
n- Hexane soluble fraction (A, 70g) Aqueous layer
Extracted with DCM
DCM soluble Aqueous layer fraction (B, 170g)
extracted with Ethyl acetate
Ethyl acetate soluble Aqueous layer fraction (C, 60g)
Extracted with Ethanol
Ethanol soluble fraction (D, 51g) Aqueous layer
Scheme 1 Extraction and Fraction of R. obtusifolius
89
DCM soluble fraction (B, 170g)
Column Chromatography
F1 F6 F5 F4 F3 F2 !00% EtOAc 100%DCM DCM:n-hex DCM:n-hex 100% n-haxane DCM:n-hex 50%:50% 75%:25% 25%:75%
Re-Chromatographed
AcOEt :DCM DCM:AcOEt DCM:AcOEt n-hexane:DCM 1:1 1:2 9:1 1:9
Compound D Compound C Compound B Compound A (Obtusifolate D) (Obtusifolate C) (Obtusifolate B) (Obtusifolate A) 105 104 103 102
Scheme 2 Chromatographic resolution on Si-gel column eluted with n-hexane, DCM and EtOAs as solvent system.
90
4.6.4. Obtusifolate A (102)
19 O OH O OH
21 18 17 1 9a 9 8a 8 O 13 6' 3 6 4a 10 10a 16 1' 5 12
4' 2' O 11 14 1'' 4'' H 5'' 2'' O 3'' Obtusifolate A (102) O 7'' 6'' 8''
Physical State: yellow amorphous solid.
UV Spectra: λmax 211, 239, 252, 275, and 366 nm
-1 IR (dry KBr) νmax cm : (3441, 3425), (1701–1728), (1590) and (1619)
Mass Spectra: HREI-MS as C39H42O8 (m/z =638.2880; calcd: 638.2870)
1 H-NMR (CDCl3, 500 MHz) δ (ppm): δ =12.31(1H, s, H-1), 7.02 (1H, s, H-4), 7.12 (1H, s, H-
7), 12.13 (1H, s, H-8), 2.38 (3H, s, H-11), 1.28 (6H, s, H-13 & H-14), 1.20 (2H ,q, H-15), 0.85
(3H, t, J=6.7Hz, H-16), 4.20 (1H, m, H-18), 1.35 (3H, d, J=6.6Hz, H-19), 1.75(2H, m, H-20),
0.92 (3H, t, J=6.7Hz, H-21), 7.66 (1H, d, J=3Hz, H- 3'), 7.72 (1H, dd, J=3 & 8.8, H-5'), 7.56
(1H, d, J=8.8, H-6'), 3.62 (2H, s, H-1''), 2.13 (3H, s, H-3'' ), 6.69(1H, s, H-5''), 1.65 (3H, s, H-
7''), 1.70 (3H, s, H-8'').
91
13 C-NMR (CDCl3, 100 MHz) δ (ppm): 165.42 (C-1), 117.00 (C-2), 138.90 (C-3), 124.50 (C-4),
144.00 (C-5), 150.13 (C-6), 144.40 (C-7), 159.00 (C-8), 190.50 (C-9), 181.00 (C-10), 134.04 (C-
4a), 114.20 (C-8a), 113.10 (C-9a), 133.15 (C-10a), 20.01 (C-11), 34.50 (C-12), 29.60 (C-13 &
C-14), 37.60 (C-15), 9.00 (C-16), 168.12 (C-17), 74.00 (C-18), 22.02 (C-19), 29.80 (C-20), 8.01
(C-21), 138.70 (C- 1'), 132.30 (C-2'), 129.40 (C-3'), 136.60 (C-4'), 127.80 (C-5'), 127.50 (C-6')
48.4 (C-1''), 206.01 (C-2''), 31.10 (C-3''), 192.10 (C-4''), 120(C-5''), 133.10 (C-6''), 18.5 (C-7''),
25.5 (C-8'').
92
4.6.5. Obtusifolate B (103)
O OH O OH 18 1 9a 9 8a 8 O 17 13 6' 3 6 10 10a 4a 16 1' 5 12 4' O 11 14 3' 7' 1'' Obtusifolate B (103) O 2'' 4'' H 3'' 5''
Physical State: yellow amorphous solid.
UV Spectra: λmax 211, 252, 275, and 366 nm
-1 -1 IR (dry KBr) νmax cm : (3441, 3425), (1701–1728), (1590) and (1619) cm
Mass Spectra: HREI-MS as C34H34O7 (m/z =554.2305; calcd.554.2296),
1 H-NMR (CDCl3, 500 MHz) δ (ppm): δ =12.31 (1H, s, H-1), 7.02 (1H, s, H-4), 7.12 (1H, s, H-
7), 12.13 (1H, s, H-8), 2.38 (3H, s, H-11), 1.28 (6H, s, H-13 & H-14), (2H, 1.20, q, H-15), 0.85
(3H, t, J=6.7Hz, H-16), 4.23 (3H, s, H-17), 7.66 (1H, d, J=3Hz, H-3'), 7.72 (1H, dd, J=3 &
8.8Hz, H-5'), 7.56 (1H, d, J=8.8, H-6'), 2.47 (3H,s,H-7'), 6.69 (1H, s, H-2''), 1.65 (3H, s, H-4''),
1.70 (3H, s, H-5'').
13 C-NMR (CDCl3, 100 MHz) δ (ppm): 165.00 (C-1), 116.01(C-2), 138.60 (C-3), 124.55 (C-4),
144.00 (C-5), 150.14 (C-6), 144.40 (C-7), 159.00 (C-8), 190.50 (C-9), 181.00 (C-10), 134.04 (C-
4a), 114.20 (C-8a), 113.10 (C-9a), 133.15 (C-10a), 20.00 (C-11), 34.50 (C-12), 29.60 (C-13 &
93
C-14), 37.60 (C-15), 9.00 (C-16), 166.10 (C-17), 51.60 (C-18), 139.50 (C- 1'), 136.70 (C-2'),
130.00 (C-3'), 136.60 (C-4'), 127.80 (C-5'), 127.50 (C-6'), 22.5 (C-7'), 192.10 (C-1''), 120.00 (C-
2''), 133.10(C-3''), 18.5 (C-4''), 25.5 (C-5'').
94
4.6.6 Obtusifolate C (104)
O 23 O 8 1 21 13 17 7 8a 9 1a O 11 18 20 12 19 O 3 5a 10 4a 5 4
O 14 O 15 Obtusifolate C(104)
16
Physical State: orange amorphous solid.
UV Spectra: λmax intense absorption at 240-260 nm, medium absorption at 320-330 nm
-1 IR (dry KBr) νmax cm : (1701–1728, 1715 and (1590)
Mass Spectra: HREI-MS as C27H28O6 (m/z= 448.1886; calcd.448.1876)
1 H-NMR (CDCl3, 500 MHz) δ (ppm): 7.57 (1H, d, J=8.8, H-3), 7.55 (1H, d, J=8.8, H-4), 7.72
(1H, d, J=3.3, H-6), 7.74 (1H, d, J=3.3, H-8), 4.23(2H, q, H-12), 1.28 (3H, t, J=6.5Hz, H-13),
3.91 (2H, s, H-14), 2.13 (3H, s, H-16), 1.35 (6H, s, H-19 & H-20), 1.42 (2H, d, H-21), 0.93 (3H, t, J=6.5Hz, H-22), 2.39 (3H, s, H-23)
13 C-NMR (CDCl3, 100 MHz) δ (ppm): 144.00 (C-1), 136.60 (C-2), 127.80 (C-3), 127.50 (C-4),
132.30 (C-5), 129.40 (C-6), 117.00 (C-7), 124.50 (C-8), 181.00 (C-9), 182.50 (C-10), 134.04 (C-
1a), 133.15 (C-8a), 132.00 (C-4a), 132.50 (C-5a), 168.12 (C-11), 72.50 (C-12), 22.70 (C-13),
95
48.40 (C-14), 206.01 (C-15), 31.30 (C-16), 209.00 (C-17), 48.40 (C-18), 22.02 (C-19 & C-20),
34.50 (C-21), 9.00 (C-22), 20.01 (C-23).
4.6.7. Obtusifolate D (105)
O 21 O 8 1 19 13 8a 9 1a O 15 11 7 16 18 12 17 O 3 5a 10 4a 5 4 Obtusifolate D (105) 14 O O
Physical State: Brown amorphous solid
UV Spectra: λmax intense absorption at 240-260 nm, medium absorption at 320-330 nm
-1 IR (dry KBr) νmax cm : (1701–1728), (1590) and (1270—1230)
Mass Spectra: HREI-MS as C25H26O6 (m/z =422.1729; calcd.422.1719).
1 H-NMR (CDCl3, 500 MHz) δ (ppm): 7.57 (1H,d, J=8.8, H-3), 7.55 (1H,d, J=8.8, H-4), 7.72
(1H, d, J=3.3, H-6), 7.74 (1H, d, J=3.3, H-8), 4.23 (2H, q, H-12), 1.28 (3H, t, J=6.5Hz, H-13),
3.79 (2H, s, H-14), 1.35 (6H, s, H-17 & H-18), 1.42 (2H, d, H-19), 0.93 (3H, t, J=6.5Hz, H-20),
2.39(3H, s, H-21).
13 C-NMR (CDCl3, 100 MHz) δ (ppm): 144.00 (C-1), 136.60 (C-2), 127.80 (C-3), 127.50 (C-4),
150.13 (C-5), 129.40 (C-6), 117.00 (C-7), 124.50 (C-8), 181.00 (C-9), 182.50 (C-10), 134.04 (C-
96
1a), 133.15 (C-8a), 132.00 (C-4a), 132.50 (C-5a), 168.12 (C-11), 72.50 (C-12), 22.70 (C-13),
56.60 (C-14), 109.00 (C-15), 48.40 (C-16), 22.02 (C-17 & C-18), 34.50 (C-19), 20.01 (C-21).
4.7. Free radical scavenging activity (RSA) of the isolated compounds
TLC-DPPH assay was used for qualitative analysis of radical scavenging screening as described in literature [178] and for quantitative estimation of radical scavenging activity (RSA) according to the standard assay [179]. In brief 2.5cm3 of 0.04% DPPH radical solution in methanol was added to each sample solution (100×10-6L) ranging from 192.50 to 6×10-6g/cm3. The mixtures were vortex-mixed and placed in dark room for half an hour. The absorbance was recorded at
517nm using spectrometer. MeOH was used as baseline control and ascorbic and gallic acid as positive controls. RSA was calculated as decrease in absorbance (samples V DPPH standard solution). %RSA was measured by the following formula. %RSA= [(A-B)/A)] ×100, where A is absorbance of control and B is absorbance of sample.
97
Chapter No 5
References
98
1. Schunko, C., Grasser, S., & Vogl, C. R. (2015). Explaining the resurgent popularity of
the wild: motivations for wild plant gathering in the Biosphere Reserve Grosses
Walsertal, Austria. Journal of ethnobiology and ethnomedicine, 11(1), 55.
2. Khan, T. H., Prasad, L., Sultana, A., & Sultana, S. (2005). Soy isoflavones inhibits the
genotoxicity of benzo (a) pyrene in Swiss albino mice. Human & experimental
toxicology, 24(3), 149-155.
3. Khan, T. H. (2012). Soy diet diminish oxidative injure and early promotional events
induced by CCl4 in rat liver. International Journal of Pharmacology, 8(1), 30-38.
4. Farnsworth, N. R. (1988). Screening plants for new medicines. Pages 83–97in EO
Wilson, ed., Biodiversity..
5. Sahreen, S., Khan, M. R., & Khan, R. A. (2010). Evaluation of antioxidant activities of
various solvent extracts of Carissa opaca fruits. Food chemistry, 122(4), 1205-1211.
6. Cragg, G. M., & Newman, D. J. (2001). Medicinals for the millennia. Annals of the New
York Academy of Sciences, 953(1), 3-25.
7. Singh, A. (2007). Herbal Medicine-Dream Unresolved. Ethnobotanical Leaflets, 2007(1),
18.
8. Sharma, A., Shanker, C., Tyagi, L. K., Singh, M., & Rao, C. V. (2008). Herbal medicine
for market potential in India: an overview. Acad J Plant Sci, 1(2), 26-36.
9. Nair, R., & Chanda, S. (2007). Antibacterial activities of some medicinal plants of the
western region of India. Turkish Journal of Biology, 31(4), 231-236.
10. Vaghasiya, Y. (2009). Screening of some medicinal Plants for Antimicrobial Properties-
Phytochemical and Pharmacological Studies of a Selected Medicinal Plant (Doctoral
dissertation, Saurashtra University).
99
11. Krishnaraju, A. V., Rao, T. V., Sundararaju, D., Vanisree, M., Tsay, H. S., & Subbaraju,
G. V. (2005). Assessment of bioactivity of Indian medicinal plants using brine shrimp
(Artemia salina) lethality assay. Int J Appl Sci Eng, 3(2), 125-34.
12. Dev, S. (1997). Ethnotherapeutics and modern drug development: the potential of
Ayurveda. Current science, 73(11), 909-928.
13. World Health Organization. (2002). WHO traditional medicine strategy 2002-2005.
14. World Health Organization. (2005). WHO global atlas of traditional, complementary and
alternative medicine (Vol. 2). World Health Organization.
15. Calixto, J. B. (2000). Efficacy, safety, quality control, marketing and regulatory
guidelines for herbal medicines (phytotherapeutic agents). Brazilian Journal of Medical
and Biological Research, 33(2), 179-189..
16. Kong, J. M., Goh, N. K., Chia, L. S., & Chia, T. F. (2003). Recent advances in traditional
plant drugs and orchids. Acta Pharmacologica Sinica, 24(1), 7-21.
17. Turker, A. U., & Usta, C. (2008). Biological screening of some Turkish medicinal plant
extracts for antimicrobial and toxicity activities. Natural product research, 22(2), 136-
146.
18. Kivçak, B., Mert, T., & Öztürk, H. T. (2002). Antimicrobial and cytotoxic activities of
Ceratonia siliqua L. extracts. Turkish Journal of Biology, 26(4), 197-200.
19. Balunas, M. J., & Kinghorn, A. D. (2005). Drug discovery from medicinal plants. Life
sciences, 78(5), 431-441.
20. Li, A. J., Bao, B., Grabovskaya-Borodina, A. E., Hong, S. P., McNeill, J., Mosyakin, S.
L., ... & Park, C. W. (2003). Polygonaceae. Flora of China, 5, 277-350.
100
21. Lajter, I. (2016). Biologically active secondary metabolites from Asteraceae and
Polygonaceae species (Doctoral dissertation, szte).
22. Hegnauer, R. (2013). Chemotaxonomie der Pflanzen: Band XIb-2: Leguminosae Teil 3:
Papilionoideae (Vol. 35). Springer-Verlag.
23. Vrchotova, N., Sera, B., & Dadáková, E. (2010). HPLC and CE analysis of catechins,
stilbens and quercetin in flowers and stems of Polygonum cuspidatum, P. sachalinense
and P. x bohemicum. Journal of the Indian Chemical Society, 87(10), 1267-1272.
24. Wood, C. E. W., Shaw, C. E., Robertson, E. A. V. K. S., & Kenneth, R. (1974). A
student's atlas of flowering plants: some dicotyledons of eastern North America (No.
Sirsi) i9780060472078).
25. Lee, N. J., Choi, J. H., Koo, B. S., Ryu, S. Y., Han, Y. H., Lee, S. I., & Lee, D. U. (2005).
Antimutagenicity and cytotoxicity of the constituents from the aerial parts of Rumex
acetosa. Biological and Pharmaceutical Bulletin, 28(11), 2158-2161.
26. Reynolds, T. (1985). The compounds in Aloe leaf exudates: a review. Botanical Journal
of the Linnean society, 90(3), 157-177.
27. Liu, S. Y., Sporer, F., Wink, M., Jourdane, J., Henning, R., Li, Y. L., & Ruppel, A.
(1997). Anthraquinones in Rheum palmatum and Rumex dentatus (Polygonaceae), and
phorbol esters in Jatropha curcas (Euphorbiaceae) with molluscicidal activity against the
schistosome vector snails Oncomelania, Biomphalaria, and Bulinus. Tropical Medicine &
International Health, 2(2), 179-188.
28. Rivero‐Cruz, I., Acevedo, L., Guerrero, J. A., Martínez, S., Pereda‐Miranda, R., Mata, R.,
... & Timmermann, B. N. (2005). Antimycobacterial agents from selected Mexican
medicinal plants. Journal of Pharmacy and Pharmacology, 57(9), 1117-1126.
101
29. Kerem, Z., Bilkis, I., Flaishman, M. A., & Sivan, L. (2006). Antioxidant Activity and
Inhibition of α-Glucosidase by trans-Resveratrol, Piceid, and a Novel trans-Stilbene from
the Roots of Israeli Rumex bucephalophorus L. Journal of agricultural and food
chemistry, 54(4), 1243-1247.
30. Fukuyama, Y., Sato, T., Asakawa, Y., & Takemoto, T. (1980). A potent cytotoxic
warburganal and related drimane-type sesquiterpenoids from Polygonum hydropiper.
Phytochemistry, 21(12), 2895-2898..
31. Asakawa, Y., & Takemoto, T. (1979). New norsesquiterpene aldehyde and sesquiterpene
hemiacetal from the seed ofPolygonum hydropiper. Experientia, 35(11), 1420-1421.
32. Haraguchi, H., Ohmi, I., Sakai, S., Fukuda, A., Toihara, Y., Fujimoto, T., ... & Yagi, A.
(1996). Effect of Polygonum hydropiper sulfated flavonoids on lens aldose reductase and
related enzymes. Journal of natural products, 59(4), 443-445.
33. Jang, D. S., Kim, J. M., Kim, J. H., & Kim, J. S. (2005). 24-nor-Ursane type triterpenoids
from the stems of Rumex japonicus. Chemical and pharmaceutical bulletin, 53(12),
1594-1596.
34. Hromádková, Z., Hirsch, J., & Ebringerová, A. (2010). Chemical evaluation of Fallopia
species leaves and antioxidant properties of their non-cellulosic polysaccharides.
Chemical Papers, 64(5), 663-672.
35. Yi, T., Zhang, H., & Cai, Z. (2007). Analysis of Rhizoma Polygoni Cuspidati by HPLC
and HPLC‐ESI/MS. Phytochemical analysis, 18(5), 387-392.
36. Lin, H. W., Sun, M. X., Wang, Y. H., Yang, L. M., Yang, Y. R., Huang, N., ... & Xiao,
K. (2010). Anti-HIV activities of the compounds isolated from Polygonum cuspidatum
and Polygonum multiflorum. Planta medica, 76(09), 889-892.
102
37. Yagi, A., Uemura, T., Okamura, N., Haraguchi, H., Imoto, T., & Hashimoto, K. (1994).
Antioxidative sulphated flavonoids in leaves of Polygonum hydropiper. Phytochemistry,
35(4), 885-887.
38. Csokay, B., Prajda, N., Weber, G., & Olah, E. (1997). Molecular mechanisms in the
antiproliferative action of quercetin. Life Sciences, 60(24), 2157-2163.
39. Yan, X. M., Joo, M. J., Lim, J. C., Whang, W. K., Sim, S. S., Im, C., ... & Sohn, U. D.
(2011). The effect of quercetin-3-O-β-D-glucuronopyranoside on indomethacin-induced
gastric damage in rats via induction of mucus secretion and down-regulation of ICAM-1
expression. Archives of pharmacal research, 34(9), 1527-1534.
40. Cho, J. H., Park, S. Y., Lee, H. S., Whang, W. K., & Sohn, U. D. (2011). The protective
effect of quercetin-3-O-β-D-glucuronopyranoside on ethanol-induced damage in cultured
feline esophageal epithelial cells. The Korean Journal of Physiology & Pharmacology,
15(6), 319-326.
41. Min, Y. S., Lee, S. E., Hong, S. T., Kim, H. S., Choi, B. C., Sim, S. S., ... & Sohn, U. D.
(2009). The inhibitory effect of quercetin-3-o-β-d-glucuronopyranoside on gastritis and
reflux esophagitis in rats. The Korean Journal of Physiology & Pharmacology, 13(4),
295-300.
42. Lee, M. J., Song, H. J., Jeong, J. Y., Park, S. Y., & Sohn, U. D. (2013). Anti-oxidative
and anti-inflammatory effects of QGC in cultured feline esophageal epithelial cells. The
Korean Journal of Physiology & Pharmacology, 17(1), 81-87.
43. Haraguchi, H., Matsuda, R., & Hashimoto, K. (1993). High-performance liquid
chromatographic determination of sesquiterpene dialdehydes and antifungal activity from
Polygonum hydropiper. Journal of agricultural and food chemistry, 41(1), 5-7.
103
44. Miyazawa, M., & Tamura, N. (2007). Inhibitory compound of tyrosinase activity from
the sprout of Polygonum hydropiper L.(Benitade). Biological and Pharmaceutical
Bulletin, 30(3), 595-597.
45. Hazarika, A., & Sarma, H. N. (2006). The estrogenic effects of Polygonum hydropiper
root extract induce follicular recruitment and endometrial hyperplasia in female albino
rats. Contraception, 74(5), 426-434.
46. Rahman, E., Goni, S. A., Rahman, M. T., & Ahmed, M. (2002). Antinociceptive activity
of Polygonum hydropiper. Fitoterapia, 73(7), 704-706.
47. Lin, M. L., Lu, Y. C., Chung, J. G., Li, Y. C., Wang, S. G., Sue-Hwee, N. G., ... & Chen,
S. S. (2010). Aloe-emodin induces apoptosis of human nasopharyngeal carcinoma cells
via caspase-8-mediated activation of the mitochondrial death pathway. Cancer letters,
291(1), 46-58.
48. Xue, J., Ding, W., & Liu, Y. (2010). Anti-diabetic effects of emodin involved in the
activation of PPARγ on high-fat diet-fed and low dose of streptozotocin-induced diabetic
mice. Fitoterapia, 81(3), 173-177.
49. Wang, Z. H., Chen, H., Guo, H. C., Tong, H. F., Liu, J. X., Wei, W. T., ... & Lin, S. Z.
(2011). Enhanced antitumor efficacy by the combination of emodin and gemcitabine
against human pancreatic cancer cells via downregulation of the expression of XIAP in
vitro and in vivo. International journal of oncology, 39(5), 1123-1131.
50. Hsu, C. M., Hsu, Y. A., Tsai, Y., Shieh, F. K., Huang, S. H., Wan, L., & Tsai, F. J.
(2010). Emodin inhibits the growth of hepatoma cells: finding the common anti-cancer
104
pathway using Huh7, Hep3B, and HepG2 cells. Biochemical and biophysical research
communications, 392(4), 473-478.
51. Du, J., Sun, L. N., Xing, W. W., Huang, B. K., Jia, M., Wu, J. Z., ... & Qin, L. P. (2009).
Lipid-lowering effects of polydatin from Polygonum cuspidatum in hyperlipidemic
hamsters. Phytomedicine, 16(6), 652-658.
52. Liu, T., Jin, H., Sun, Q. R., Xu, J. H., & Hu, H. T. (2010). Neuroprotective effects of
emodin in rat cortical neurons against β-amyloid-induced neurotoxicity. Brain research,
1347, 149-160.
53. Saleh, N. A., El-Hadidi, M. N., & Arafa, R. F. (1993). Flavonoids and anthraquinones of
some Egyptian Rumex species (Polygonaceae). Biochemical systematics and ecology,
21(2), 301-303.
54. Rao, K. N. V., Ch, S., & Banji, D. (2011). A study on the nutraceuticals from the genus
Rumex. Hygeia.J.D.Med.vol.3 (1), 2011, 76- 88.
55. Oswald, A. K., & Haggar, R. J. (1983). The effects of Rumex obtusifolius on the seasonal
yield of two mainly perennial ryegrass swards. Grass and Forage Science, 38(3), 187-
191.
56. Courtney, A. D. (1985). Impact and control of docks in grassland. Weeds, pests and
diseases of grasslands and herbage legumes, 120-127.
57. Klimeš, L., Klimešová, J., & Osbornová, J. (1993). Regeneration capacity and
carbohydrate reserves in a clonal plant Rumex alpinus: effect of burial. Vegetatio, 153-
160.
58. Richards, J. H., & Lee, D. W. (2002). " To See... Heaven in a Wild Flower...": Teaching
Botany in the 21st Century.
105
59. Europaea, F. (1993). Tutin TG, Heywood VH, Burges NA, Valentine DH, Walters SM,
Webb DA, editors.
60. Hejduk, S., & Dolezal, P. (2004). Nutritive value of broad-leaved dock (Rumex
obtusifolius L.) and its effect on the quality of grass silages. Czech Journal of Animal
Science-UZPI (Czech Republic).
61. Gledhill, D. (2008). The names of plants. Cambridge University Press.
62. DiTomaso, J. M., Kyser, G. B., Oneto, S. R., Wilson, R. G., Orloff, S. B., Anderson, L.
W., ... & Ransom, C. (2013). Weed control in natural areas in the Western United States.
63. Pye, A. (2008). Ecological studies of Rumex crispus L (Vol. 2008, No. 101).
64. Anjen, L., Grabovskaya-Borodina, A. E., & Mosyakin, S. L. (2003). Rumex. Flora of
china, 5, 333-341.
65. Pardo-De-Santayana, M., Tardío, J., & Morales, R. (2005). The gathering and
consumption of wild edible plants in the Campoo (Cantabria, Spain). International
Journal of Food Sciences and Nutrition, 56(7), 529-542.
66. Giday, M., Asfaw, Z., & Woldu, Z. (2009). Medicinal plants of the Meinit ethnic group
of Ethiopia: an ethnobotanical study. Journal of Ethnopharmacology, 124(3), 513-521.
67. Cakilcioglu, U., & Turkoglu, I. (2010). An ethnobotanical survey of medicinal plants in
Sivrice (Elazığ-Turkey). Journal of Ethnopharmacology, 132(1), 165-175.
68. Alfawaz, M. A. (2006). Chemical composition of hummayd (Rumex vesicarius) grown in
Saudi Arabia. Journal of food composition and analysis, 19(6), 552-555.
69. Pardo-de-Santayana, M., Tardío, J., Blanco, E., Carvalho, A. M., Lastra, J. J., San
Miguel, E., & Morales, R. (2007). Traditional knowledge of wild edible plants used in the
106
northwest of the Iberian Peninsula (Spain and Portugal): a comparative study. Journal of
Ethnobiology and Ethnomedicine, 3(1), 27.
70. Łuczaj, Ł., & Szymański, W. M. (2007). Wild vascular plants gathered for consumption
in the Polish countryside: a review. Journal of Ethnobiology and Ethnomedicine, 3(1), 17.
71. Cakilcioglu, U. (2009). Ethnobotanical features of Citli Lowland (Elazig) and its vicinity.
Ecological Life Sciences, 4(2), 81-85.
72. Łuczaj, Ł. (2010). Changes in the utilization of wild green vegetables in Poland since the
19th century: a comparison of four ethnobotanical surveys. Journal of
ethnopharmacology, 128(2), 395-404.
73. Polat, R., Cakilcioglu, U., Ertug, F., & Satil, F. (2012). An evaluation of ethnobotanical
studies in Eastern Anatolia. Biological Diversity and Conservation, 5(2), 23-40.
74. Łuczaj, Ł., Köhler, P., Pirożnikow, E., Graniszewska, M., Pieroni, A., & Gervasi, T.
(2013). Wild edible plants of Belarus: from Rostafiński’s questionnaire of 1883 to the
present. Journal of ethnobiology and ethnomedicine, 9(1), 21.
75. Sõukand, R., & Kalle, R. (2015). Emic conceptualization of a'wild edible plant'in Estonia
in the second half of the 20th century. Trames: A Journal of the Humanities and Social
Sciences, 19(1), 15.
76. Dénes, A., Papp, N., Babai, D., Czúcz, B., & Molnár, Z. (2013). Edible wild plants and
their use based on ethnographic and ethnobotanical researches among Hungarian in the
Carpathian Basin. Dunántúli Dolgozatok (A) Természettudományi Sorozat, 13, 35-76.
77. Nedelcheva, A. (2013). An ethnobotanical study of wild edible plants in Bulgaria.
EurAsian Journal of BioSciences, 7, 77-94.
107
78. Guerra, L., Pereira, C., Andrade, P. B., Rodrigues, M. A., Ferreres, F., Pinho, P. G. D., ...
& Valentão, P. (2008). Targeted metabolite analysis and antioxidant potential of Rumex
induratus. Journal of agricultural and food chemistry, 56(17), 8184-8194.
79. Moerman, D. (2003). Native American ethnobotany. A database of foods, drugs, dyes
and fibers of Native American peoples, derived from plants. University of Michigan-
Dearborn. Online at http://herb. umd. umich. edu/Accessed, 1(3), 07.
80. Ali-Shtayeh, M. S., Jamous, R. M., Al-Shafie, J. H., Elgharabah, W. A., Kherfan, F. A.,
Qarariah, K. H., ... & Herzallah, H. M. (2008). Traditional knowledge of wild edible
plants used in Palestine (Northern West Bank): a comparative study. Journal of
Ethnobiology and Ethnomedicine, 4(1), 13.
81. Misra, S., Maikhuri, R. K., Kala, C. P., Rao, K. S., & Saxena, K. G. (2008). Wild leafy
vegetables: A study of their subsistence dietetic support to the inhabitants of Nanda Devi
Biosphere Reserve, India. Journal of Ethnobiology and Ethnomedicine, 4(1), 15.
82. Dreon, A. L., & Paoletti, M. G. (2009). The wild food (plants and insects) in Western
Friuli local knowledge (Friuli-Venezia Giulia, North Eastern Italy). Contributions to
Natural History, 12, 461-488.
83. Lewis, W. H., & Elvin-Lewis, M. P. (2003). Medical botany: plants affecting human
health. John Wiley & Sons.
84. Abbet, C., Mayor, R., Roguet, D., Spichiger, R., Hamburger, M., & Potterat, O. (2014).
Ethnobotanical survey on wild alpine food plants in Lower and Central Valais
(Switzerland). Journal of ethnopharmacology, 151(1), 624-634.
85. Pareek, A., & Kumar, A. (2014). Rumex crispus L.–A plant of traditional value. Drug
Discovery, 9(20), 20-23.
108
86. Št’astná, P., Klimeš, L., & Klimešová, J. (2010). Biological flora of Central Europe:
Rumex alpinus L. Perspectives in Plant Ecology, Evolution and Systematics, 12(1), 67-
79.
87. Dogan, Y., Nedelcheva, A., Łuczaj, Ł., Drăgulescu, C., Stefkov, G., Maglajlić, A., ... &
Dajić-Stevanović, Z. (2015). Of the importance of a leaf: the ethnobotany of sarma in
Turkey and the Balkans. Journal of ethnobiology and ethnomedicine, 11(1), 26.
88. Mekonnen, T., Urga, K., & Engidawork, E. (2010). Evaluation of the diuretic and
analgesic activities of the rhizomes of Rumex abyssinicus Jacq in mice. Journal of
ethnopharmacology, 127(2), 433-439.
89. Munavu, R. M., Mudamba, L. O., & Ogur, J. A. (1984). Isolation and characterization of
the major anthraquinone pigments from Rumex abysinica. Planta medica, 50(01), 111-
111.
90. Bélanger, J., Balakrishna, M., Latha, P., Katumalla, S., & Johns, T. (2010). Contribution
of selected wild and cultivated leafy vegetables from South India to lutein and β-carotene
intake. Asia Pacific journal of clinical nutrition, 19(3), 417-424.
91. Taylor, R. S. L., Hudson, J. B., Manandhar, N. P., & Towers, G. H. N. (1996). Antiviral
activities of medicinal plants of southern Nepal. Journal of Ethnopharmacology, 53(2),
105-110.
92. Demirezer, L. Ö., Kuruüzüm-Uz, A., Bergere, I., Schiewe, H. J., & Zeeck, A. (2001). The
structures of antioxidant and cytotoxic agents from natural source: anthraquinones and
tannins from roots of Rumex patientia. Phytochemistry, 58(8), 1213-1217.
109
93. Kisangau, D. P., Hosea, K. M., Lyaruu, H. V., Joseph, C. C., Mbwambo, Z. H., Masimba,
P. J., ... & Sewald, N. (2009). Screening of traditionally used Tanzanian medicinal plants
for antifungal activity. Pharmaceutical biology, 47(8), 708-716.
94. Gautam, R., Karkhile, K. V., Bhutani, K. K., & Jachak, S. M. (2010). Anti-inflammatory,
cyclooxygenase (COX)-2, COX-1 inhibitory, and free radical scavenging effects of
Rumex nepalensis. Planta medica, 76(14), 1564-1569.
95. Liang, H. X., Dai, H. Q., Fu, H. A., Dong, X. P., Adebayo, A. H., Zhang, L. X., & Cheng,
Y. X. (2010). Bioactive compounds from Rumex plants. Phytochemistry Letters, 3(4),
181-184.
96. Lee, H. S., Kim, S. K., Han, J. B., Choi, H. M., Park, J. H., Kim, E. C., ... & Min, B. I.
(2006). Inhibitory effects of Rumex japonicus Houtt. on the development of atopic
dermatitis‐like skin lesions in NC/Nga mice. British Journal of Dermatology, 155(1), 33-
38.
97. Tyler, V. E. (1992). The honest herbal: a sensible guide to the use of herbs and related
remedies.
98. Grieve, Maude. "A Modern Herbal, Available online http://botanical. com/NOTE: Much
of Mrs. Grieve’s text is based on traditional knowledge and much has been disproven."
Do not use as medical advice, but rather as historical information (1931).
99. Butură, V. (1979). Romanian ethnobotany encyclopedia. The Scientific and Encyclopedic
Publishing, Bucharest, Romania
100. Allen, D. E., & Hatfield, G. (2004). Medicinal plants in folk tradition. Timber
Press.
110
101. Vogl, S., Picker, P., Mihaly-Bison, J., Fakhrudin, N., Atanasov, A. G., Heiss, E.
H., ... & Kopp, B. (2013). Ethnopharmacological in vitro studies on Austria's folk
medicine—An unexplored lore in vitro anti-inflammatory activities of 71 Austrian
traditional herbal drugs. Journal of ethnopharmacology, 149(3), 750-771.
102. Getie, M., Gebre-Mariam, T., Rietz, R., Höhne, C., Huschka, C., Schmidtke, M.,
... & Neubert, R. H. H. (2003). Evaluation of the anti-microbial and anti-inflammatory
activities of the medicinal plants Dodonaea viscosa, Rumex nervosus and Rumex
abyssinicus. Fitoterapia, 74(1), 139-143.
103. Ahmad, S. S., Erum, S., Khan, S. M., Nawaz, M., & Wahid, A. (2014). Exploring
the medicinal plants wealth: a traditional medico-botanical knowledge of local
communities in Changa Manga Forest, Pakistan. Middle-East J. Sci. Res, 20(12), 1772-
1779.
104. VanderJagt, T. J., Ghattas, R., VanderJagt, D. J., Crossey, M., & Glew, R. H.
(2002). Comparison of the total antioxidant content of 30 widely used medicinal plants of
New Mexico. Life Sciences, 70(9), 1035-1040.
105. de Dieu Tamokou, J., Chouna, J. R., Fischer-Fodor, E., Chereches, G., Barbos, O.,
Damian, G., ... & Kuiate, J. R. (2013). Anticancer and antimicrobial activities of some
antioxidant-rich Cameroonian medicinal plants. PLoS One, 8(2), e55880.
106. Lone, I. A., Kaur, G., Athar, M., & Alam, M. S. (2007). Protective effect of
Rumex patientia (English Spinach) roots on ferric nitrilotriacetate (Fe-NTA) induced
hepatic oxidative stress and tumor promotion response. Food and chemical toxicology,
45(10), 1821-1829.
111
107. Elzaawely, A. A., Xuan, T. D., & Tawata, S. (2005). Antioxidant and antibacterial
activities of Rumex japonicus HOUTT. Aerial parts. Biological and Pharmaceutical
Bulletin, 28(12), 2225-2230.
108. Morales, P., Ferreira, I. C., Carvalho, A. M., Sánchez-Mata, M. D. C., Cámara,
M., & Tardío, J. (2012). Fatty acids profiles of some Spanish wild vegetables. Revista de
Agaroquimica y Tecnologia de Alimentos, 18(3), 281-290.
109. Khan, T. H., Ganaie, M. A., Siddiqui, N. A., Alam, A., & Ansari, M. N. (2014).
Antioxidant potential of Rumex vesicarius L.: in vitro approach. Asian Pacific journal of
tropical biomedicine, 4(7), 538-544.
110. Sahreen, S., Khan, M. R., & Khan, R. A. (2014). Comprehensive assessment of
phenolics and antiradical potential of Rumex hastatus D. Don. roots. BMC
complementary and alternative medicine, 14(1), 47.
111. Abbasi, A. M., Shah, M. H., Li, T., Fu, X., Guo, X., & Liu, R. H. (2015).
Ethnomedicinal values, phenolic contents and antioxidant properties of wild culinary
vegetables. Journal of ethnopharmacology, 162, 333-345.
112. Yıldırım, A., Mavi, A., & Kara, A. A. (2001). Determination of antioxidant and
antimicrobial activities of Rumex crispus L. extracts. Journal of agricultural and food
chemistry, 49(8), 4083-4089.
113. Suh, H. J., Lee, K. S., Kim, S. R., Shin, M. H., Park, S., & Park, S. (2011).
Determination of singlet oxygen quenching and protection of biological systems by
various extracts from seed of Rumex crispus L. Journal of Photochemistry and
Photobiology B: Biology, 102(2), 102-107.
112
114. Shiwani, S., Singh, N. K., & Wang, M. H. (2012). Carbohydrase inhibition and
anti-cancerous and free radical scavenging properties along with DNA and protein
protection ability of methanolic root extracts of Rumex crispus. Nutrition research and
practice, 6(5), 389-395.
115. Humeera, N., Kamili, A. N., Bandh, S. A., Lone, B. A., & Gousia, N. (2013).
Antimicrobial and antioxidant activities of alcoholic extracts of Rumex dentatus L.
Microbial pathogenesis, 57, 17-20.
116. Ferreres, F., Ribeiro, V., Izquierdo, A. G., Rodrigues, M. Â., Seabra, R. M.,
Andrade, P. B., & Valentão, P. (2006). Rumex induratus leaves: interesting dietary
source of potential bioactive compounds. Journal of agricultural and food chemistry,
54(16), 5782-5789.
117. Wegiera, M. A. G. D. A. L. E. N. A., Smolarz, H. D., & Bogucka-Kocka, A. N.
N. A. (2012). Rumex L. species induce apoptosis in 1301, EOL-1 and H-9 cell lines. Acta
poloniae pharmaceutica, 69(3), 487-99.
118. Lajter, I., Zupkó, I., Molnár, J., Jakab, G., Balogh, L., Vasas, A., & Hohmann, J.
(2013). Antiproliferative activity of Polygonaceae species from the Carpathian Basin
against human cancer cell lines. Phytotherapy Research, 27(1), 77-85.
119. Demirezer, Ö. L., & Kuruüzüm, A. (1997). Rapid and simple biological activity
screening of some Rumex species; evaluation of bioguided fractions of R. scutatus and
pure compounds. Zeitschrift für Naturforschung C, 52(9-10), 665-669.
120. Harshaw, D., Nahar, L., Vadla, B., & Sarker, S. D. (2010). Bioactivity of Rumex
obtusifolius (Polygonaceae). Archives of Biological Sciences, 62(2), 387-392.
113
121. Zhang, H., Guo, Z., Wu, N., Xu, W., Han, L., Li, N., & Han, Y. (2012). Two
novel naphthalene glucosides and an anthraquinone isolated from Rumex dentatus and
their antiproliferation activities in four cell lines. Molecules, 17(1), 843-850.
122. Jayasuriya, H., Koonchanok, N. M., Geahlen, R. L., McLaughlin, J. L., & Chang,
C. J. (1992). Emodin, a protein tyrosine kinase inhibitor from Polygonum cuspidatum.
Journal of Natural Products, 55(5), 696-698.
123. Zhang, L., Chang, C. J., Bacus, S. S., & Hung, M. C. (1995). Suppressed
transformation and induced differentiation of HER-2/neu-overexpressing breast cancer
cells by emodin. Cancer research, 55(17), 3890-3896.
124. Lee, N. J., Choi, J. H., Koo, B. S., Ryu, S. Y., Han, Y. H., Lee, S. I., & Lee, D. U.
(2005). Antimutagenicity and cytotoxicity of the constituents from the aerial parts of
Rumex acetosa. Biological and Pharmaceutical Bulletin, 28(11), 2158-2161.
125. Hasan, A., Ahmed, I., Jay, M., & Voirin, B. (1995). Flavonoid glycosides and an
anthraquinone from Rumex chalepensis. Phytochemistry, 39(5), 1211-1213.
126. Abd, E. F. H., Gohar, A., El-Dahmy, S., & Hubaishi, A. (1994). Phytochemical
investigation of Rumex luminiastrum. Acta pharmaceutica Hungarica, 64(3), 83-85.
127. Wegiera, M. A. G. D. A. L. E. N. A., Smolarz, H. D., Wianowska, D. O. R. O. T.
A., & Dawidowicz, A. L. (2007). Anthracene derivatives in some species of Rumex L.
genus. Acta Societatis Botanicorum Poloniae, 76(2).
128. Mei, R., Liang, H., Wang, J., Zeng, L., Lu, Q., & Cheng, Y. (2009). New seco-
anthraquinone glucosides from Rumex nepalensis. Planta medica, 75(10), 1162-1164.
114
129. Başkan, S., Daut-Özdemir, A., Günaydın, K., & Erim, F. B. (2007). Analysis of
anthraquinones in Rumex crispus by micellar electrokinetic chromatography. Talanta,
71(2), 747-750.
130. Gunaydin, K., Topcu, G., & Ion, R. M. (2002). 1, 5-Dihydroxyanthraquinones and
an anthrone from roots of Rumex crispus. Natural product letters, 16(1), 65-70.
131. Jiang, L., Zhang, S., & Xuan, L. (2007). Oxanthrone C-glycosides and
epoxynaphthoquinol from the roots of Rumex japonicus. Phytochemistry, 68(19), 2444-
2449.
132. Yang, Y., Yan, Y. M., Wei, W., Luo, J., Zhang, L. S., Zhou, X. J., ... & Cheng, Y.
X. (2013). Anthraquinone derivatives from Rumex plants and endophytic Aspergillus
fumigatus and their effects on diabetic nephropathy. Bioorganic & medicinal chemistry
letters, 23(13), 3905-3909.
133. Zhu, J. J., Zhang, C. F., Zhang, M., Bligh, S. A., Yang, L., Wang, Z. M., & Wang,
Z. T. (2010). Separation and identification of three epimeric pairs of new C-glucosyl
anthrones from Rumex dentatus by on-line high performance liquid chromatography–
circular dichroism analysis. Journal of Chromatography A, 1217(33), 5384-5388.
134. Zee, O. P., Kim, D. K., Kwon, H. C., & Lee, K. R. (1998). A new
epoxynaphthoquinol from Rumex japonicus. Archives of pharmacal research, 21(4), 485-
486.
135. Zhang, L. S., Li, Z., Mei, R. Q., Liu, G. M., Long, C. L., Wang, Y. H., & Cheng,
Y. X. (2009). Hastatusides A and B: two new phenolic glucosides from Rumex hastatus.
Helvetica Chimica Acta, 92(4), 774-778.
115
136. Nishina, A., Kubota, K., & Osawa, T. (1993). Antimicrobial components,
trachrysone and 2-methoxystypandrone, in Rumex japonicus Houtt. Journal of
agricultural and food chemistry, 41(10), 1772-1775.
137. Demirezer, L. Ö., Kuruüzüm-Uz, A., Bergere, I., Schiewe, H. J., & Zeeck, A.
(2001). The structures of antioxidant and cytotoxic agents from natural source:
anthraquinones and tannins from roots of Rumex patientia. Phytochemistry, 58(8), 1213-
1217.
138. Kuruüzüm, A., Demirezer, L. Ö., Bergere, I., & Zeeck, A. (2001). Two New
Chlorinated Naphthalene Glycosides from Rumex p atientia. Journal of natural products,
64(5), 688-690.
139. El‐Hawary, S. A., Sokkar, N. M., Ali, Z. Y., & Yehia, M. M. (2011). A profile of
bioactive compounds of Rumex vesicarius L. Journal of food science, 76(8).
140. Aritomi, M.,Kiyota,I.,Mazaki,T., (1965). Flavonoid constituents in leaves of
Rumex acetosa Linnaeus and R. japonicus Houttuyn. Chemical & pharmaceutical
bulletin, 13(12), 1470-1471.
141. Stöggl, W. M., Huck, C. W., & Bonn, G. K. (2004). Structural elucidation of
catechin and epicatechin in sorrel leaf extracts using liquid‐chromatography coupled to
diode array‐, fluorescence‐, and mass spectrometric detection. Journal of separation
science, 27(7‐8), 524-528.
142. Gescher, K., Hensel, A., Hafezi, W., Derksen, A., & Kühn, J. (2011). Oligomeric
proanthocyanidins from Rumex acetosa L. inhibit the attachment of herpes simplex virus
type-1. Antiviral research, 89(1), 9-18.
116
143. Bicker, J., Petereit, F., & Hensel, A. (2009). Proanthocyanidins and a
phloroglucinol derivative from Rumex acetosa L. Fitoterapia, 80(8), 483-495.
144. Kerem, Z., Regev-Shoshani, G., Flaishman, M. A., & Sivan, L. (2003).
Resveratrol and Two Monomethylated Stilbenes from Israeli Rumex b ucephalophorus
and Their Antioxidant Potential. Journal of natural products, 66(9), 1270-1272.
145. Molnár, P., Ősz, E., Zsila, F., & Deli, J. (2005). Isolation and structure elucidation
of anhydroluteins from cooked sorrel (Rumex rugosus CAMPD.). Chemistry &
biodiversity, 2(7), 928-935.
146. Yoon, H. M., Park, J. Y., Oh, M. H., Kim, K. H., Han, J. H., & Whang, W. K.
(2005). A new acetophenone of aerial parts from Rumex aquatica. Natural Product
Sciences, 11(2), 75-78.
147. Kucekova, Z., Mlcek, J., Humpolicek, P., Rop, O., Valasek, P., & Saha, P. (2011).
Phenolic compounds from Allium schoenoprasum, Tragopogon pratensis and Rumex
acetosa and their antiproliferative effects. Molecules, 16(11), 9207-9217.
148. Lee, J. Y., Lee, J. G., Sim, S. S., Whang, W. K., & Kim, C. J. (2011). Anti-
asthmatic effects of phenylpropanoid glycosides from Clerodendron trichotomum leaves
and Rumex gmelini herbes in conscious guinea-pigs challenged with aerosolized
ovalbumin. Phytomedicine, 18(2), 134-142.
149. Tavares, L., Carrilho, D., Tyagi, M., Barata, D., Serra, A. T., Duarte, C. M. M., ...
& Espírito-Santo, M. D. (2010). Antioxidant capacity of Macaronesian traditional
medicinal plants. Molecules, 15(4), 2576-2592.
150. Duke, J. A., & Beckstrom-Sternberg, S. M. (1994). Dr. Duke's phytochemical and
ethnobotanical databases.
117
151. Girault, L. (1984). Kallawaya, guérisseurs itinérants des Andes: recherches sur les
pratiques médicinales et magiques (No. 107). IRD Editions.
152. Kasai, T., Okuda, M., & Sakamura, S. (1981). 6-O-Malonyl-β-methyl-D-
glucopyranoside from roots of Rumex obtusifolius. Phytochemistry, 20(5), 1131-1132.
153. Haslett, B. G., Bailey, C. J., Ramshaw, J. A., Scawen, M. D., & Boulter, D.
(1978). The amino acid sequence of plastocyanin from Rumex obtusifolius.
Phytochemistry, 17(4), 615-617.
154. Ibáñez-Calero, S. L., Jullian, V., & Sauvain, M. (2009). A new anthraquinone
isolated from Rumex obtusifolius. Revista Boliviana de Química, 26(2), 49-56.
155. Spencer, P., Sivakumaran, S., Fraser, K., Foo, L. Y., Lane, G. A., Edwards, P. J.,
& Meagher, L. P. (2007). Isolation and characterisation of procyanidins from Rumex
obtusifolius. Phytochemical analysis, 18(3), 193-203.
156. Teuscher, E., & Lindequist, U. (1994). Biogene Gifte. Stuttgart etc.: Fischer.
157. Han, Y. S., Van der Heijden, R., & Verpoorte, R. (2001). Biosynthesis of
anthraquinones in cell cultures of the Rubiaceae. Plant Cell, Tissue and Organ Culture,
67(3), 201-220.
158. Hegnauer, R. (1959). CHEMOTAXONOMISCHE BETRACHTUNGEN. Planta
medica, 7(04), 344-366.
159. Thomson, R. H. (1991). Distribution of naturally occurring quinones. Pharmacy
World & Science, 13(2), 70-73.
160. Harborne, J. B. (1999). Classes and functions of secondary products from plants.
Chemicals from plants, 1-25.
118
161. Meyer, B. N., Ferrigni, N. R., Putnam, J. E., Jacobsen, L. B., Nichols, D. J., &
McLaughlin, J. L. (1982). Brine shrimp: a convenient general bioassay for active plant
constituents. Planta medica, 45(05), 31-34.
162. Harding, W. W., Henry, G. E., Lewis, P. A., Jacobs, H., McLean, S., & Reynolds,
W. F. (1999). Alvaradoins A− D. Anthracenone C Arabinosides from Alvaradoa
jamaicensis. Journal of natural products, 62(1), 98-101.
163. Schripsema, J., & Dagnino, D. (1996). Elucidation of the substitution pattern of 9,
10-anthraquinones through the chemical shifts of peri-hydroxyl protons. Phytochemistry,
42(1), 177-184.
164. Manojlovic, N. T., Solujic, S., Sukdolak, S., & Krstic, L. (2000). Isolation and
antimicrobial activity of anthraquinones from some species of the lichen genus
Xanthoria. JOURNAL-SERBIAN CHEMICAL SOCIETY, 65(8), 555-560.
165. Bizuayehu, Z. Phytochemical Investigation On The Root of Rumex Abyssinicus
(Makmako).
166. Harbone, J. B. (1998). Photochemical methods 3rd ed.
167. Parekh, J., & Chanda, S. (2007b). Antibacterial and phytochemical studies on
twelve species of Indian medicinal plants. African Journal of Biomedical Research, 10(2)
168. Surmaghi, M. S., Amin, Y. A. G., & Mahmoodi, Z. (1992). Survey of Iranian
plants for saponins alkaloids flavonoids and tannins. IV. DARU Journal of
Pharmaceutical Sciences, 2(2-3), 1-11.
169. Patharajan, S., & Balaabirami, S. (2014). Antioxidant activity and phytochemical
analysis of fractionated leaf extracts of Catharanthus roseus. Int J Pharm, 1(2), 138-143.
119
170. Segelman, A. B., Farnsworth, N. R., & Quimby, M. W. (1969). Biological and
phytochemical evaluation of plants. 3. False-negative saponin test results induced by the
presence of tannins. Lloydia, 32(1), 52.
171. Ajaiyeoba, E. O. (2002). Phytochemical and antibacterial properties of Parkia
biglobosa and Parkia bicolor leaf extracts. African Journal of Biomedical Research, 5(3).
172. Kapoor, L. D., Singh, A., Kapoor, S. L., & Srivastava, S. N. (1969). Survey of
Indian plants for saponins, alkaloids and flavonoids. I. Lloydia, 32, 297-304.
173. Bayer, A. W., Kirby, W. M. M., Sherris, J. C., & Turck, M. (1966). Antibiotic
susceptibility testing by a standardized single disc method. Am J clin pathol, 45(4), 493-
496.
174. Cruickshank, R. Medical Microbiology, A guide to diagnosis and control of
infection. 1968; E. and S. Livingstone Ltd., Edinburgh and London, 888.
175. Choudhary, M. I., Parveen, Z., Jabbar, A., & Ali, I. (1995). Antifungal steroidal
lactones from Withania coagulance. Phytochemistry, 40(4), 1243-1246.
176. Meyer-Alber, A., Hartmann, H., Stümpel, F., & Creutzfeldt, W. (1992).
Mechanism of insulin resistance in CCl 4-induced cirrhosis of rats. Gastroenterology,
102(1), 223-229.
177. Khabir, A., Khan, F., Afzal, M., Haq, Z. U., Ullah, M. A., Shah, A. M. H., ... &
Khan, S. (2017). Antimicrobial Efficacy and Cytotoxic Screening of Dichloromethane
Sub-fractions of Rumex obtusifolius. Asian Journal of Chemistry, 29(2), 367.
178. Takao, T., Kitatani, F., Watanabe, N., Yagi, A., & Sakata, K. (1994). A simple
screening method for antioxidants and isolation of several antioxidants produced by
120
marine bacteria from fish and shellfish. Bioscience, Biotechnology, and Biochemistry,
58(10), 1780-1783.
179. Mahato, S. B., & Kundu, A. P. (1994). 13C NMR spectra of pentacyclic
triterpenoids—a compilation and some salient features. Phytochemistry, 37(6), 1517-
1575.
121