Research Article | Open Access
Armelle T. Mbaveng, Francois Damen, James D. Simo Mpetga, Maurice D. Awouafack, Pierre Tane, Victor Kuete, Thomas Efferth, "Cytotoxicity of Crude Extract and Isolated Constituents of the Dichrostachys cinerea Bark towards Multifactorial Drug-Resistant Cancer Cells", Evidence-Based Complementary and Alternative Medicine, vol. 2019, Article ID 8450158, 11 pages, 2019. https://doi.org/10.1155/2019/8450158
Cytotoxicity of Crude Extract and Isolated Constituents of the Dichrostachys cinerea Bark towards Multifactorial Drug-Resistant Cancer Cells
The effectiveness of anticancer chemotherapy is greatly impeded by the resistance of malignant cells to cytotoxic drugs. In this study, the cytotoxicity of the crude extract (DCB) and compounds isolated from the bark of Dichrostachys cinerea, namely, betulinic acid (1), glyceryl-1-hexacosanoate (2), 7-hydroxy-2-(4-hydroxyphenyl)-4H-chromen-4-one (3), and 6-hydroxy-2-(4-hydroxyphenyl)-4H-chromen-4-one (4), was investigated. The study was extended to the assessment of the mode of induction of apoptosis by DCB and compound 1. The resazurin reduction assay was used for cytotoxicity studies. Assessments of cell cycle distribution, apoptosis, mitochondrial membrane potential (MMP), and reactive oxygen species (ROS) were performed by flow cytometry. Constituents of DCB were isolated by column chromatography. Triterpenoid 1 and flavone 4 had cytotoxic effects towards the 9 tested cancer cell lines with IC50 values below 50 μM. The recorded IC50 values varied from 7.65 μM (towards multidrug-resistant CEM-ADR5000 leukemia cells) to 44.17 μM (against HepG2 hepatocarcinoma cells) for 1, 18.90 μM (CCRF-CEM leukemia cells) to 88.86 μM (against HCT116p53+/+ colon adenocarcinoma cells) for 4, and 0.02 μM (against CCRF-CEM cells) to 122.96 μM (against CEM/ADR5000 cells) for doxorubicin. DCB induced apoptosis in CCRF-CEM cells mostly mediated by MMP alteration and enhanced ROS production; compound 1 induced apoptosis through caspases activation and MMP alteration and increased ROS production. Dichrostachys cinerea is an interesting cytotoxic plant and deserves more studies leading to new antineoplastic agents to fight cancer and mostly leukemia.
Recent data from the World Health Organization revealed that most countries still face an increase in cancer incidences . The global cancer burden reached 18.1 million new cases in 2018, with one in eight men and one in 11 women dying in developing countries . Worldwide, the five-year prevalence of cancer is estimated at 43.8 million people . The effectiveness of anticancer chemotherapy is greatly impeded by the resistance of malignant cells to cytotoxic drugs . The search for new antiproliferative drugs should therefore take into consideration the ability of cancer cells to develop resistant phenotypes. Natural products are well recognized as source of cytotoxic molecules . Various studies have previously documented the effectiveness of botanicals and phytochemicals from the flora of Africa to fight cancer multidrug resistance (MDR) [4, 5]. However, research should be intensified to increase the library of cytotoxic plants and molecules available in the African flora, in order to have better chances of achieving clinically exploitable drugs in the future. The present study was hence designed to evaluate the cytotoxicity of crude extract and compounds from the bark of Dichrostachys cinerea (L.) Wight & Arn. (Fabaceae) towards a panel of drug-sensitive and drug-resistant cancer cell lines. The mode of induction of apoptosis of crude extract and compound 1 was further investigated. Dichrostachys cinerea, also known as sicklebush, Bell mimosa, Chinese lantern tree, or Kalahari Christmas tree, is a fast growing tree of up to 7 m height, traditionally used as laxative, diuretic and to treat dysentery, elephantiasis, gonorrhoea, boils, headache, syphilis, sore, worms [6, 7], inflammation, and cancer . Previous phytochemical analysis of Dichrostachys cinerea led to the identification of a triterpenoid β-amyrin glucoside, apigenin-7-O-apiosyl (1→2) glucoside, chrysoeriol-7-O-apiosyl (1→2) glucoside, clovamide, quercetin-3-O-rhamnopyranoside, quercetin-3-O-glucopyranoside, myricetin-3-O-rhamnopyranoside, myricetin-3-O-glucopyranoside, myricetin, apigenin, and kaempferol from the leaves [6, 9] as well as the meroterpene derivatives, dichrostachines A-R from the bark and roots . Preliminary cytotoxicity investigations of this plant were reported towards DU145 and 22Rv1 prostate cancer cells and HeLa cervical cancer cells . This is the first intensive study on the potential of Dichrostachys cinerea and some of its constituents against MDR cancer cell lines.
2. Materials and Methods
2.1. Plant Material and Extraction
Dichrostachys cinerea barks were collected in February 2017 in Bazou (5° 4′ 0′′ N, 10° 28′ 0′′ E) in the West Region of Cameroon. The plant was identified at the National Herbarium of Cameroon (Yaoundé), where voucher is available under number 34028/HNC. The bark of D. cinerea was air-dried and powdered (2000 g) and then macerated in 20 l of ethanol for 48 h. The solvent was evaporated in vacuum under reduced pressure to give the crude extract (170 g; DCB).
2.2. Isolation of Compounds from the Bark of Dichrostachys cinerea
An aliquot of DCB (160 g) was treated with ethyl acetate (EtOAc) to give two subextracts: the EtOAc extract (DCA, 85g) and the methanol (MeOH) extract (DCB, 75g). DCA (85 g) was submitted to a silica gel flash column chromatography (CC) using dichloromethane (CH2Cl2)-EtOAc and EtOAc-MeOH mixtures of increasing polarity. Fractions of 150 ml each were collected as follows: CH2Cl2 100% (sub-frs 1-8), CH2Cl2-EtOAc 95:5 (sub-frs 9-19), CH2Cl2-EtOAc 90:10 (sub-frs 20-23), CH2Cl2-EtOAc 80:20 (sub-frs 24-30), CH2Cl2-EtOAc 60:40 (sub-frs 31-35), CH2Cl2-EtOAc 50:50 (sub-frs 36-40), EtOAc100% (sub-frs 41-45), EtOAc- MeOH 95:20 (sub-frs 46-52), EtOAc-MeOH 90:10 (sub-frs 53-60), EtOAc-MeOH 80:20 (sub-frs 61-64), EtOAc-MeOH 70:30 (sub-frs 65-68), and MeOH 100% (sub-frs 69-72). These fractions were then pooled on the basis of their analytical thin layer chromatography (TLC) profiles into five fractions (frs) as follows: DCA1 (Sub-frs 1-6; 10 g), DCA2 (Sub-frs 7-14; 12 g), DCA3 (Sub-frs 15-30; 13 g), DCA4 (Sub-frs 31-60; 20 g), and DCA5 (Sub-frs 61-72; 25 g). From a direct filtration of fraction DCA2, followed by further Sephadex CC, compound 1 was obtained as a white powder (1 g).
An aliquot of DCA5 (18 g) was submitted to silica gel flash CC using CH2Cl2-EtOAc and EtOAc-MeOH mixtures of increasing polarity. 110 subfractions (sub-frs) of 150 ml each were collected as follows: CH2Cl2100% (sub-frs 1-22), CH2Cl2-EtOAc 95:5 (sub-frs 23-53), CH2Cl2-EtOAc 90:10 (sub-frs 54-59), CH2Cl2-EtOAc 85:15 (sub-frs 60-75), CH2Cl2-EtOAc 80:20 (sub-frs 76-83), CH2Cl2-EtOAc 75:25 (sub-frs 84-91), CH2Cl2-EtOAc 70:30 (sub-frs 92-95), CH2Cl2-EtOAc 60:40 (sub-frs 96-100), EtOAc100% (sub-frs 101-104), EtOAc-MeOH 90:10 (sub-frs 105-107), and MeOH 100% (sub-frs 108-110). Compound 3 was obtained as a white powder (14 mg) in sub-frs 27-31; sub-frs 30-35 afforded compound 2 as yellow powder (15 mg); meanwhile, sub-frs 37-44 yielded compound 4 as yellow powder (15 mg).
2.3. General Procedure
All general chemistry procedures (mass spectral data, 1H and 13C nuclear magnetic resonance (NMR) spectra) and CC were performed with the same apparatus and reagents, and in similar experimental conditions as reported earlier .
2.4. Cell Cultures
Drug-sensitive and drug-resistant cancer cell lines of previously reported origin were used in this study. These included drug-sensitive CCRF-CEM leukemia cells and its multidrug-resistant P-glycoprotein-overexpressing subline CEM/ADR5000 cells [14–16], MDA-MB-231-pcDNA breast cancer cells and their resistant subline MDA-MB-231-BCRP clone 23 cells , HCT116 p53+/+colon cancer cells and their knockout clone HCT116 p53−/− cells, and U87.MG glioblastoma cells and their resistant subline U87.MGΔEGFR cells [18, 19]. Normal AML12 hepatocytes were used and compared with HepG2 hepatocarcinoma cells [18, 19].
2.5. Cytotoxicity Assay
The cytotoxicity assay performed using resazurin reduction assay was applied to the crude extract (DCB), compounds 1-4, and doxorubicin [18, 20, 21] with similar experimental conditions as those reported earlier [13, 19, 22, 23]. The Infinite M2000 Pro™ plate reader (Tecan, Crailsheim, Germany) with excitation wavelength of 544 nm and an emission wavelength of 590 nm was used to read the fluorescence after 72 h incubation. IC50 values earlier defined  were calculated from a calibration curve by linear regression using Microsoft Excel . The degree of resistance (D.R.) was determined as the IC50 value of the resistant cell line versus that of its sensitive congeners; meanwhile, the selectivity index (S.I.) was the IC50 value in normal AML12 hepatocytes versus that in HepG2 hepatocarcinoma.
2.6. Cell Cycle Analysis and Detection of Apoptotic Cells by Flow Cytometry and Annexin V/PI Staining
Aliquots of 1×106 CCRF-CEM cells were treated with the studied samples (DCB and compound 1), the reference drug (doxorubicin), or the solvent control (DMSO) at various concentrations. The distribution of CCRF-CEM cycle was analyzed as described earlier in similar experimental conditions (24 h incubation; humidified 5% CO2 atmosphere; 37°C) [13, 22, 23]. The BD Accuri C6 Flow Cytometer (BD Biosciences, Heidelberg, Germany) was used to measure the propidium iodide (PI) fluorescence of individual nuclei. Assays were repeated at least three times and in triplicate.
To perform the annexin V/PI staining, DCB, betulinic acid (1), and doxorubicin were used to treat an amount of 1×106 per 1 ml CCRF-CEM cells. The experimental conditions were similar to those earlier reported (24 h incubation; humidified 5% CO2 atmosphere; 37°C) . The BD Accuri C6 Flow Cytometer was then used to analyze apoptosis using fluorescein isothiocyanate (FITC)-conjugated annexin V/PI assay kit (eBioscience™ Annexin V; Invitrogen, San Diego, USA) similarly as reported earlier [13, 22, 23]; early apoptosis for cells stained with only annexin V; late apoptosis or in a necrotic stage for cells stained with both annexin V and propidium iodide [13, 25, 26].
2.7. Assessment of Caspases Activation Using the Caspase-Glo Assay
After 6 h treatment of CCRF-CEM cells with DCB and triterpenoid 1 for 6 h, caspases activities were evaluated with Caspase-Glo 3/7, 8, and 9 assay kits (Promega, Mannheim, Germany) similarly as previously reported [13, 18, 27].
2.8. Assessment of the Integrity of the Mitochondrial Membrane
The mitochondrial membrane potential (MMP) of CCRF-CEM cells was analyzed after 24 h treatment with DCB, compound 1, or valinomycin (mitochondrial gradient dissipation substance or positive control). The 5,5′,6,6′-tetrachloro-1,1′,3,3′-tetraethylbenzimidazolyl carbocyanine iodide (JC-1; Biomol, Hamburg, Germany) staining was used to measure the MMP similarly as previously reported [13, 18, 22, 23].
2.9. Evaluation of the Production of Reactive Oxygen Species (ROS)
The measurement of ROS production using 2′,7′-dichlorodihydrofluorescein diacetate (H2DCFH-DA) (Sigma-Aldrich) was done in CCRF-CEM cells were treated with DCB, compound 1, a solvent control (DMSO), or a positive control, hydrogen peroxide (H2O2) for 24 h, in similar experimental conditions as documented earlier [13, 18, 28, 29].
Physical and NMR data with direct comparison with literature was used to elucidate the chemical structures of phytochemicals isolated from the bark of Dichrostachys cinerea. They were betulinic acid, C30H50O (1; m.p. 216°C; m/z 426) , glyceryl-1-hexacosanoate, C29H58O4 (2; m.p. 91-93°C; m/z 470) , 7-hydroxy-2-(4-hydroxyphenyl)-4H-chromen-4-one, C15H10O4 (3; m.p. 315°C; m/z 254) , and 6-hydroxy-2-(4-hydroxyphenyl)-4H-chromen-4-one, C15H10O4 (4; m.p. 325°C; m/z 254 )  (Figure 1).
Triterpenoid 1 and flavone 4 had cytotoxic effects towards the 9 tested cancer cell lines with IC50 values below 50 μM (Table 1). Botanical DCB and flavone 3 had selective activities, while no cytotoxic effect (IC50 value above 100 μM) was recorded with fatty acid ester 2. The recorded IC50 values varied from 7.65 μM (towards resistant CEM-ADR5000 leukemia cells) to 44.17 μM (against HepG2 hepatocarcinoma cells) for 1, 18.90 μM (CCRF-CEM leukemia cells) to 88.86 μM (against HCT116p53+/+ colon adenocarcinoma cells) for 4, and 0.02 μM (against CCRF-CEM cells) to 122.96 μM (against CEM/ADR5000 cells) for doxorubicin. The IC50 values in normal AML12 hepatocytes were above 80 μg/mL for DCB and above 100 μM for compounds 2 and 3 (Table 1). Collateral sensitivity (hypersensitivity or D.R. below 1) of all resistant cell lines compared to their sensitive counterparts was observed with triterpenoid 1 (Table 1). Hypersensitivity or normal sensitivity of at least one resistant cell line to botanical DCB as well as compounds 3 and 4 was also recorded (Table 1). Selectivity indexes above 2 were also observed with compound 1 (S.I.: >2.13) and doxorubicin (S.I.: 11.59) in HepG2 as compared with normal AML12 hepatocytes (Table 1).
(): the degree of resistance was determined as the ratio of value in the resistant divided by the in the sensitive cell line; CEM/ADR5000, MDA-MB-231-BCRP, HCT116 (p53-/-), and U87MG.ΔEGFR were used as the corresponding resistant counterparts for CCRF-CEM, MDA-MB-231-pcDNA, HCT116 (p53+/+), and U87MG, respectively; (): the selectivity index was determined as the ratio of value in the normal AML12 hepatocytes divided by the in HepG2 hepatocarcinoma cells. In bold: significant cytotoxic effect [4, 11, 12]; (): values in μg/mL; (): values in μM; (nd): not determined;1: betulinic acid; 2: glyceryl-1-hexacosanoate; 3: 7-hydroxy-2-(4-hydroxyphenyl)-4H-chromen-4-one; and 4: 6-hydroxy-2-(4-hydroxyphenyl)-4H-chromen-4-one.
3.3. Cell Cycle Distribution and Apoptosis
Upon treatment of CCRF-CEM cells with botanical DCB, triterpenoid 1, and the reference compound doxorubicin, the cell cycle phases were modified in concentration-dependent manner (Figure 2). Increase of cells in sub-G0/G1 phase was observed with all samples, and DCB induced cell cycle arrest in G0/G1 phase, while triterpenoid 1 caused cycle arrest in G2/M; doxorubicin induced arrest of cell cycle between S and G2/M. The percentage of CCRF-CEM cells in sub-G0/G1 phase in nontreated cells only was 1.78%; meanwhile, it varied upon treatment from 4.00% (1/4 × IC50) to 32.18% (2 × IC50) for DCB, 15.30% (1/4 × IC50) to 48.40% (2 × IC50) for compound 1, and 4.81% (1/4 × IC50) to 10.35% (2 × IC50) for doxorubicin (Figure 2). These data suggested that DCB, compound 1, and doxorubicin induced apoptosis in CCRF-CEM cells. In the annexin V/PI staining, the induction of apoptosis was further investigated. The results depicted in Figure 3 showed a dose-dependent induction with DCB, triterpenoid 1, and doxorubicin. When cells were treated with 2 × IC50, for example, DCB induced apoptosis with 39.8% early apoptotic V (+)/PI (-) cells, 8.8% late apoptotic V (+)/PI (+) cells as well as necrosis with 12.8% annexin V (-)/PI (+) cells; triterpenoid 1 induced 51.0% early apoptotic cells and 5.1% necrotic cells, while doxorubicin induced 11.8% late apoptotic cells.
3.4. Activation of Caspases, Integrity of MMP, and ROS Production
Treatment of CCRF-CEM cells with DCB did not activate the activity of caspases 3/7, 8, and 9 contrary to triterpenoid 1 (Figure 4). In effect, a dose-dependent activation of caspases upon treatment with 1 was observed, with optimal effects at 8.8 μM; up to 3.19-fold, 2.91-fold, and 2.37-fold increases in the activity of caspases 3/7, 8, and 9, respectively, were recorded.
The effects of DCB, betulinic acid (1), and valinomycin on integrity of MMP in CCRF-CEM are depicted in Figure 5. Both DCB and compound 1 considerably modified the MMP with up to 90.3% and 57.5% (at 2 × IC50), respectively; valinomycin at 10 μM induced 45.9% alteration.
The effects of DCB and compound 1 on the production of ROS in CCRF-CEM cells are given in Figure 6. The two samples dose-dependently enhanced the production of ROS in CCRF-CEM cells. The ROS level in nontreated cells was 0.2%, whilst at 2 × IC50, DCB caused increased ROS production by up to 61.1% and triterpenoid 1 by 53.30%. H2O2 induced ROS production by 98.8% at 50 μM.
Phytochemicals isolated from the bark of Dichrostachys cinerea were one triterpenoid 1, one ester of fatty acid 2, and two flavone-type flavonoids 3 and 4. Previous phytochemical investigation of the bark of Dichrostachys cinerea led to the isolation of meroterpene derivatives, dichrostachines A-R  which were not isolated in this study, probably due to the isolation procedure used or the fact that the plant was harvested in different geographic locations.
Drug resistance of malignant cells seriously hampers the chemotherapy of cancer. In the search for cytotoxic compounds, scientists should take into consideration the ability of these cells to rapidly develop drug resistance. This is possible when investigations also consider resistant phenotypes of malignant cells. In the present study, we have used several models of MDR cancer cell lines including ATP-binding cassette (ABC)-transporter-overexpressing MDR-mediating P-glycoprotein (P-gp; ABCB1/MDR1) or breast cancer resistance protein (ABCG2/BCRP), a p53 knockout cell line, and a mutation-activated EGFR gene (ΔEGFR) cell line. The resistant P-gp overexpressing CEM/ADR5000 cells treated with the crude extract DCB were collaterally sensitive  compared to their sensitive parental subline CCRF-CEM cells (Table 1). Hypersensitivity of all resistant cell lines to betulinic acid as compared to their respective sensitive counterparts was also observed; for flavones 3 and 4, the hypersensitivity or otherwise normally sensitive (D.R. below or around 1) of at least three resistant cell lines was also recorded. Generally, the D.Rs. recorded upon treatments with DCB, compounds 1, 3, and 4 were lower than with doxorubicin (Table 1). Previous studies also reported the hypersensitivity of CEM/ADR5000 leukemia cells to compound 1 as compared to its sensitive congener CCRF-CEM cells . These data are indications that Dichrostachys cinerea and its constituents have the potential to combat cancer multidrug resistance. According to the National Cancer Institute USA (NCI), good botanicals should exert their cytotoxicity with IC50 values below 20 μg/ml upon 48 h or 72 h incubation , while this set point is 10 μM for phytochemicals [11, 12]. Also, NCI recommends that botanicals yielding IC50 values below or around 30 μg/ml should undergo purification to isolate cytotoxic molecules . In this work, IC50 values as low as 4.69 μg/ml and 4.13 μg/ml were recorded with the crude extract DCB, on both sensitive and resistant leukemia cells, respectively (Table 1). Selective and lower IC50 values were recorded with DCB on carcinoma cells, clearly indicating that this plant could likely be used to combat leukemia. This was also the case with betulinic acid (1), as IC50 values below 10 μM were also recorded towards leukemia cells, and higher values obtained in carcinoma cells. Though flavones 3 and 4 had cytotoxic effects in several cell lines including leukemia and carcinoma phenotypes, all IC50 values obtained were above 10 μM. This confirms the hypothesis that this plant and its constituents could mostly be used in the fight against leukemia. The good S.I. (>2) of compound 1 also indicates that it can be used in chemotherapy (Table 1). In effect, the low cytotoxicity of betulinic acid towards the normal PBL peripheral blood lymphoblast was also reported . However, its lower S.I. as compared to that of doxorubicin, clinically associated with many adverse effects to patients (despite higher S.I.), clearly indicates that further studies on the toxicity of this compound as well as the crude extract will be necessary.
To the best of our knowledge, this is the first intensive study on cytotoxicity of Dichrostachys cinerea and its constituents 3 and 4 against MDR cancer cell lines. However, preliminary antiproliferative effects of this plant were reported towards DU145 and 22Rv1 prostate cancer cells and HeLa cervical cancer cells, with the lowest IC50 values of 8.04 μg/ml recorded in 22Rv1 cells . Also, betulinic acid is a well-known cytotoxic compound . Its effects have been reported towards several cancer cell lines including sensitive and resistant phenotypes such as CCRF-CEM cells and CEM/ADR5000 leukemia cells, MDA-MB-231-pcDNA and MDA-MB-231/BCRP breast adenocarcinoma cells, HEK293 and HEK293/ABCB5 embryonic kidney cells, and U87.MG and U87.MGΔEGFR glioblastoma cells with IC50 values ranging from 15.1 μM (against HEK293 cells) to 29.4 μM (towards CCRF-CEM cells) [34, 36].
In this study, the crude extract DCB and triterpenoid 1 had the best cytotoxic effects on the two leukemia cells with IC50 values below 10 μM. They were consequently selected for further cellular mechanistic studies towards CCRF-CEM cells, such as induction of apoptosis, caspases activation, and alteration of MMP as well as the production of ROS . DCB and compound 1 induced apoptosis in CCRF-CEM cells (Figures 2 and 3). Induction of apoptosis by DCB was mediated by MMP alteration and increased ROS production, while that induced by triterpenoid 1 was mediated by caspases activation (Figure 4), MMP alteration (Figure 5), and increased ROS production (Figure 6). Previous studies on the molecular mechanism of the cytotoxic action of compound 1 showed that it inhibited P-gp, BCRP, and ABCB5 and mutation activated EGFR overexpressing cells. Besides, various genes significantly correlated to its activity on cell cycle regulation, microtubule formation, signal transduction, transcriptional regulation, chromatin remodeling, cell adhesion, tumor suppression, ubiquitination, and proteasome degradation .
The present study indicated that Dichrostachys cinerea is a potential cytotoxic plant and should be further explored to develop new antineoplastic agents to fight recalcitrant cancers. The crude extract DCB induced apoptosis in CCRF-CEM cells mostly mediated by MMP alteration and enhanced ROS production; compound 1 induced apoptosis through caspases activation and MMP alteration and increased ROS production.
|BCRP:||Breast cancer resistance protein|
|DCB:||Crude extract from the bark of Dichrostachys cinerea|
|D.R.:||Degree of resistance|
|EGFR:||Epidermal growth factor receptor|
|ESI-MS:||Electrospray ionization mass spectrometry|
|IC50:||50% inhibitory concentration|
|MMP:||Mitochondrial membrane potential|
|NMR:||Nuclear magnetic resonance|
|ROS:||Reactive oxygen species|
|TLC:||Thin layer chromatography|
The data used to support the findings of this study are included within the article.
Conflicts of Interest
The authors declare that there are no conflicts of interest regarding the publication of this paper.
Armelle T. Mbaveng and Francois Damen carried out the experiments. Victor Kuete, Pierre Tane, and Thomas Efferth designed the study. Maurice D. Awouafack performed NMR experiments. Francois Damen, Maurice D. Awouafack, and James D. Simo Mpetga contributed to structural elucidation. Armelle T. Mbaveng and Victor Kuete wrote the manuscript. Thomas Efferth supervised the work, corrected the manuscript, and provided the facilities for the study. All authors read and approved the final manuscript.
Funding was provided by the Alexander von Humboldt (AvH) foundation (Grant no.: CMR 1163890 GF-E to ATM). Armelle T. Mbaveng is thankful to AvH Foundation for an 18-month fellowship in Prof. Dr. Thomas Efferth’s Laboratory in Mainz, Germany, through the “Georg Foster Research Fellowship for Experienced Researcher” program. ATM is also grateful to the AvH Foundation for the return fellowship to the University of Dschang. Authors are also thankful to the Institute of Molecular Biology gGmbH (IMB) (Mainz, Germany), where the flow cytometry experiments were performed.
Supplementary file.docx. RMN 1H, 13C and major chemical shifts of studied compounds, betulinic acid (1), glyceryl-1-hexacosanoate (2), 7-hydroxy-2-(4-hydroxyphenyl)-4H-chromen-4-one (3), and 6-hydroxy-2-(4-hydroxyphenyl)-4H-chromen-4-one (4). (Supplementary Materials)
- IARC, “Latest global cancer data: cancer burden rises to 18.1 million new cases and 9.6 million cancer deaths in 2018,” Tech. Rep., International Agency for Research on Cancer, 2018.
- C. Fitzmaurice, D. Dicker, A. Pain et al., “The global burden of cancer 2013,” JAMA Oncology, vol. 1, no. 4, pp. 505–527, 2015.
- N. P. Gullett, A. R. M. Ruhul Amin, S. Bayraktar et al., “Cancer prevention with natural compounds,” Seminars in Oncology, vol. 37, no. 3, pp. 258–281, 2010.
- V. Kuete and T. Efferth, “African flora has the potential to fight multidrug resistance of cancer,” BioMed Research International, vol. 2015, Article ID 914813, 24 pages, 2015.
- A. T. Mbaveng, V. Kuete, and T. Efferth, “Potential of central, Eastern and Western Africa medicinal plants for cancer therapy: spotlight on resistant cells and molecular targets,” Frontiers in Pharmacology, vol. 8, p. 343, 2017.
- R. T. El-Sharawy, A. Elkhateeb, M. M. Marzouk, R. R. Abd El-Latif, S. E. Abdelrazig, and M. A. El-Ansari, “Antiviral and antiparasitic activities of clovamide: the major constituent of Dichrostachys cinerea (L.) wight et arn,” Journal of Applied Pharmaceutical Science, vol. 7, no. 9, pp. 219–223, 2017.
- P. M. Kimani, P. G. Mwitari, S. Mwenda Njagi, P. Gakio Kirira, and D. M. Kiboi, “In vitro anti-proliferative activity of selected plant extracts against cervical and prostate cancer cell lines,” Journal of Cancer Science & Therapy, vol. 10, no. 9, 2018.
- G. F. Ibikunle, S. K. Okwute, and E. O. Ogbadoyi, “Cytotoxic agents from nigerian plants: a case study of Spondias mombin Linn (Anacardiaceae) leaves,” FUW Trends in Science & Technology Journal, vol. 2, no. 1B, pp. 510–513, 2017.
- M. Vijayalakshmi, K. Periyanayagam, K. Kavitha, and K. Akilandeshwari, “Phytochemical analysis of ethanolic extract of Dichrostachys Cinerea W and Arn leaves by a thin layer chromatography, high performance thin layer chromatography and column chromatography,” Ancient Science of Life, vol. 32, no. 4, pp. 227–233, 2013.
- C. Long, L. Marcourt, R. Raux et al., “Meroterpenes from Dichrostachys cinerea inhibit protein farnesyl transferase activity,” Journal of Natural Products, vol. 72, no. 10, pp. 1804–1815, 2009.
- J. Boik, Natural Compounds in Cancer Therapy, Oregon Medical Press, Minnesota, Minn, USA, 2001.
- G. Brahemi, F. R. Kona, A. Fiasella et al., “Exploring the structural requirements for inhibition of the ubiquitin E3 ligase breast cancer associated protein 2 (BCA2) as a treatment for breast cancer,” Journal of Medicinal Chemistry, vol. 53, no. 7, pp. 2757–2765, 2010.
- A. T. Mbaveng, F. Damen, İ. Çelik, P. Tane, V. Kuete, and T. Efferth, “Cytotoxicity of the crude extract and constituents of the bark of Fagara tessmannii towards multi-factorial drug resistant cancer cells,” Journal of Ethnopharmacology, vol. 235, pp. 28–37, 2019.
- A. Kimmig, V. Gekeler, M. Neumann et al., “Susceptibility of multidrug-resistant human leukemia cell lines to human interleukin 2-activated killer-cells,” Cancer Research, vol. 50, no. 21, pp. 6793–6799, 1990.
- T. Efferth, A. Sauerbrey, A. Olbrich et al., “Molecular modes of action of artesunate in tumor cell lines,” Molecular Pharmacology, vol. 64, no. 2, pp. 382–394, 2003.
- J.-P. Gillet, T. Efferth, D. Steinbach et al., “Microarray-based detection of multidrug resistance in human tumor cells by expression profiling of ATP-binding cassette transporter genes,” Cancer Research, vol. 64, no. 24, pp. 8987–8993, 2004.
- L. A. Doyle, W. Yang, L. V. Abruzzo et al., “A multidrug resistance transporter from human MCF-7 breast cancer cells,” Proceedings of the National Acadamy of Sciences of the United States of America, vol. 95, no. 26, pp. 15665–15670, 1998.
- V. Kuete, L. P. Sandjo, J. L. N. Ouete, H. Fouotsa, B. Wiench, and T. Efferth, “Cytotoxicity and modes of action of three naturally occurring xanthones (8-hydroxycudraxanthone G, morusignin i and cudraxanthone I) against sensitive and multidrug-resistant cancer cell lines,” Phytomedicine, vol. 21, no. 3, pp. 315–322, 2014.
- V. Kuete, A. T. Mbaveng, L. P. Sandjo, M. Zeino, and T. Efferth, “Cytotoxicity and mode of action of a naturally occurring naphthoquinone, 2-acetyl-7-methoxynaphtho[2,3-b]furan-4,9-quinone towards multi-factorial drug-resistant cancer cells,” Phytomedicine, vol. 33, pp. 62–68, 2017.
- J. O'Brien, O. Wilson, T. Orton, and F. Pognan, “Investigation of the Alamar blue (resazurin) fluorescent dye for the assessment of mammalian cell cytotoxicity,” European Journal of Biochemistry, vol. 267, no. 17, pp. 5421–5426, 2000.
- V. Kuete, P. D. Tchakam, B. Wiench et al., “Cytotoxicity and modes of action of four naturally occuring benzophenones: 2,2′,5,6′-Tetrahydroxybenzophenone, guttiferone E, isogarcinol and isoxanthochymol,” Phytomedicine, vol. 20, no. 6, pp. 528–536, 2013.
- A. T. Mbaveng, B. L. Ndontsa, V. Kuete et al., “A naturally occuring triterpene saponin ardisiacrispin B displayed cytotoxic effects in multi-factorial drug resistant cancer cells via ferroptotic and apoptotic cell death,” Phytomedicine, vol. 43, pp. 78–85, 2018.
- A. T. Mbaveng, G. W. Fotso, D. Ngnintedo et al., “Cytotoxicity of epunctanone and four other phytochemicals isolated from the medicinal plants Garcinia epunctata and Ptycholobium contortum towards multi-factorial drug resistant cancer cells,” Phytomedicine, vol. 48, pp. 112–119, 2018.
- J. Dzoyem, A. NKuete, V. Kuete et al., “Cytotoxicity and antimicrobial activity of the methanol extract and compounds from Polygonum limbatum,” Planta Medica, vol. 78, no. 8, pp. 787–792, 2012.
- D. A. Gerwirtz and L. W. Elmore, “Apoptosis as the predominant tumor cell response to chemotherapy and irradiation: a case of TUNEL vision?” Current Opinion in Investigational Drugs, vol. 6, no. 12, p. 1199, 2005.
- S. Samarghandian, J. T. Afshari, and S. Davoodi, “Chrysin reduces proliferation and induces apoptosis in the human prostate cancer cell line pc-3,” Clinics, vol. 66, no. 6, pp. 1073–1079, 2011.
- V. Kuete, L. P. Sandjo, D. E. Djeussi et al., “Cytotoxic flavonoids and isoflavonoids from Erythrina sigmoidea towards multi-factorial drug resistant cancer cells,” Investigational New Drugs, vol. 32, no. 6, pp. 1053–1062, 2014.
- D. A. Bass, J. W. Parce, L. R. Dechatelet, P. Szejda, M. C. Seeds, and M. Thomas, “Flow cytometric studies of oxidative product formation by neutrophils: a graded response to membrane stimulation,” Journal of Immunology, vol. 130, no. 4, pp. 1910–1917, 1983.
- A. Cossarizza, R. Ferraresi, L. Troiano et al., “Simultaneous analysis of reactive oxygen species and reduced glutathione content in living cells by polychromatic flow cytometry,” Nature Protocols, vol. 4, no. 12, pp. 1790–1797, 2009.
- S. B. Mahato and A. P. Kundu, “13C NMR Spectra of pentacyclic triterpenoids—a compilation and some salient features,” Phytochemistry, vol. 37, no. 6, pp. 1517–1575, 1994.
- R. N. Mbouangouere, P. Tane, D. Ngamga, P. Djemgou, M. I. Choudhary, and B. T. Ngadjui, “Piptaderol from Piptadenia africana,” African Journal of Traditional, Complementary and Alternative Medicines, vol. 4, no. 3, pp. 294–298, 2007.
- A. O. Oladimeji, I. A. Oladosu, M. S. Ali, and Z. Ahmed, “Flavonoids from the roots of Dioclea reflexa (Hook F.),” Bulletin of the Chemical Society of Ethiopia, vol. 29, no. 3, pp. 441–448, 2015.
- H. Yoon, S. Eom, J. Hyun et al., “1H and 13C NMR data on hydroxy/methoxy flavonoids and the effects of substituents on chemical shifts,” Bulletin of the Korean Chemical Society, vol. 32, no. 6, pp. 2101–2104, 2011.
- M. E. M. Saeed, N. Mahmoud, Y. Sugimoto, T. Efferth, and H. Abdel-Aziz, “Betulinic acid exerts cytotoxic activity against multidrug-resistant tumor cells via targeting autocrine motility factor receptor (AMFR),” Frontiers in Pharmacology, vol. 9, p. 418, 2018.
- M. Suffness and J. Pezzuto, “Assays related to cancer drug discovery,” in Methods in Plant Biochemistry: Assays for Bioactivity, K. Hostettmann, Ed., pp. 71–133, Academic Press, London, UK, 1990.
- V. Zuco, R. Supino, S. C. Righetti et al., “Selective cytotoxicity of betulinic acid on tumor cell lines, but not on normal cells,” Cancer Letters, vol. 175, no. 1, pp. 17–25, 2002.
- Y. Fuchs and H. Steller, “Programmed cell death in animal development and disease,” Cell, vol. 147, no. 4, pp. 742–758, 2011.
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