Chemo-resistance is the main factor for poor prognosis in human ovarian epithelial cancer. Active constituents derived from Chinese medicine with anti-cancer potential might circumvent this obstacle. In our present study, evodiamine (EVO) derived from Evodia rutaecarpa (Juss.) Benth suppressed the proliferation of human epithelial ovarian cancer, A2780 and the related paclitaxel-resistant cell lines and did not cause cytotoxicity, as confirmed by the significant decline of clone formation and the representative alterations of CFDA-SE fluorescence. Meanwhile, EVO induced cell cycle arrest in a dose- and time-dependent manner. This disturbance might be mediated by the cooperation of Cyclin B1 and Cdc2, including the up-regulation of Cyclin B1, p27 and p21 and activation failure of Cdc2 and pRb. MAPK signaling pathway regulation also assisted in this process. Furthermore, chemo-sensitivity potential was enhanced as indicated in A2780/PTXR cells by the down-regulation of MDR-1 expression, accompanied by MDR-1 function suppression. Taken together, we confirmed initially that EVO exerted an anti-proliferative effect on human epithelial ovarian cancer cells, A2780/WT and A2780/PTXR, induced G2/M phase cell cycle arrest and improved chemo-resistance. Overall, we found that EVO significantly suppressed malignant proliferation in human epithelial ovarian cancer, thus proving to be a potential anti-cancer agent in the future.
Chemo-resistance is the main factor for poor prognosis in human ovarian epithelial cancer. As a result, since the year 2000 when X-linked inhibitors for apoptotic proteins (Xiap) assisted by p53 status were regarded as important targets for chemo-resistance in human ovarian epithelial cancer1, extensive investigations have concentrated on Xiap and the PI3K/Akt pathway2,3, BRCA1/2 alterations4, epithelial mesenchymal transition and cancerous ovarian stem cells5,6 and even considered metabolic alterations and epigenetic therapies7,8, in order to circumvent chemo-resistance.
Cell division cycle protein 2 (Cdc2) or cyclin-dependent kinase 1 (Cdk1) leads the entry into M phase and is also a key regulator in cell cycle progression by binding to cyclin kinases and causing phosphorylation. Over-expressed Cdc2 phosphorylating survivin has been found to be one of the causes of paclitaxel-resistant ovarian cancer9. For example, a reduction of Cdc2 was induced by down-regulation of BRCA1, which conferred paclitaxel resistance in breast cancer cells10. An inappropriate activation of Cdc2 induced by cyclin A1 contributed to an apoptotic and mitotic catastrophe in ovarian cancer11. Cdc2 siRNA also increased the sensitivity to cisplatin-induced apoptosis in ovarian cancer cells12. The phosphorylation inhibition of Cdc2 at Tyr 15 mediated DNA damage in UHRF1 (ubiquitin-like PHD and RING finger domain-containing 1) depletion ovarian cancer cells13.
Cyclin B1 is another important regulatory protein in the cell cycle and it interacts with Cdc2 to form the cyclin B1-Cdk1 complex, promoting mitotic initiation14. These proteins prefer to over-express in low-malignant-potential tumors rather than epithelial ovarian cancer to develop tumorigenesis15. Cyclin binding and phosphorylation activation at Thr161 of Cdc2 are both required for Cdc2 activation for mitosis in cell cycle progression. p27 is a cyclin-dependent kinase inhibitor which binds to Cdc2 to prevent cell cycle transition. p27 and p21 are regarded as potential tumor suppressors and low levels of p27 and high levels of phospho-Rb were found to significantly correlate with poor patient survival in ovarian cancer16. Rb is another signature for human high-grade serous epithelial ovarian cancer17 and it is phosphorylated by cyclin D kinases to lead to progression into the S phase of the cell cycle18. ERK and p38 are the main factors in the MAPK pathway, which also regulates cell cycle distribution in ovarian cancer. The Ras pathway is mutated in low-grade serous ovarian carcinomas19 where resistant cells are characterized by activation of the Ras/ERK pathway20. P-glycoprotein (P-gp) expression and function are also clinically significant in patients with ovarian cancer therapy21.
Evodiamine (EVO) is an indole alkaloid derived from Chinese medicine, Evodia rutaecarpa (Juss.) Benth. Reports show that it exerts anti-cancer potential in a wide range of cancer cell lines, including non-small-cell cancer cells, osteosarcoma cells, lung cancer cells, glioblastoma cells, etc. The mechanisms involved were found to suppress malignant proliferation, induce cell cycle arrest and inhibit invasion and metastasis22,23,24,25,26,27,28,29,30,31,32,33,34,35,36,37,38,39,40,41,42,43,44. However, there is no report on human epithelial ovarian cancer cells and the related chemo-resistant cancer cells. Therefore, our present study was designed to investigate the effect of EVO on chemo-sensitive and -resistant human epithelial ovarian cancer and the underlying mechanisms.
Materials and Methods
EVO, paclitaxel (PTX), crystal violet and 3-[4,5-dimethyl-2-thiazolyl]-2,5-diphenyl tetrazolium bromide (MTT) were purchased from Sigma-Aldrich (St. Louis, MO). Dulbecco’s Modified Eagle Medium (DMEM), fetal bovine serum (FBS), penicillin (100 U/ml)-streptomycin (100 μg/ml), phosphate-buffered saline (PBS) and 0.25% w/v trypsin/1 mM EDTA from Gibco Life Technologies (Grand Island, USA) were used for cell culture. Calcium AM and carboxyfluorescein diacetate succinimidyl ester (CFDA-SE) were purchased from Molecular Probes (Grand Island, USA). The lactate dehydrogenase (LDH) release detection kit was purchased from Roche Diagnostics (Mannheim, Germany). The primary and secondary antibodies against Cyclin B1, p27, p21, Rb, p-Cdc2 (Thr161), Cdc2, p-ERK (Thr202/Tyr204), ERK, p38, Ras, GAPDH and β-actin were purchased from Cell Signaling Technology (Danvers, MA). MDR-1 was obtained from Santa Cruz (Santa Cruz, USA).
Cell lines and Cell culture
Human ovarian epithelial cancer cells, A2780/WT were used for anti-proliferation study. The paclitaxel-resistant A2780 cells were established by stepwise exposure to increased concentrations of paclitaxel, as previously described45. Cells were cultured in RPMI 1640 medium with penicillin (100 U/ml)-streptomycin (100 μg/ml) and 10% (v/v) FBS at 37 °C in a humidified atmosphere of 5% CO2.
MTT assay and LDH assay
The MTT assay was conducted for cell viability investigation as previously described46. A2780/WT cells and A2780/PTXR cells were seeded in 96-well plates at a final concentration of 5 ×103 cells/well. After a 24-hour incubation for adhesion, cells were treated with EVO at a series of concentrations. After a 24-hour incubation, cell viability was incubated with MTT solution (1 mg/ml) for four hours. The formazan crystal formation was dissolved with DMSO and determined by absorbance at 570 nm using a micro-plate reader (SpectraMax M5, Molecular Devices). Cell viability was expressed as a percentage of the vehicle control. The LDH release from cells after EVO treatment was determined with a commercial kit according to the manufacturers’ protocol (Roche). The percentage of LDH release was calculated as per our previous reports47.
A2780/WT and A2780/PTXR cells were exposed to different doses of EVO for 24 hours. After the indicated treatments, cell morphology was observed and captured using a microscope (Olympus MVX10, Japan) equipped with a digital camera (ColorView II, Soft Imaging System, Olympus), to survey cell counts and morphology alteration at 100 × magnification. The representative images were based on at least three independent experiments.
Colony formation assay
Cells were plated in 6-well plates with 5 × 102 cells per well in duplicate. After a 15-day incubation at 37 °C for visible colonies, these colonies were fixed with 4% paraformaldehyde for 15 minutes and stained with crystal violet for five minutes. The number of colonies (≥50 cells as a colony) was captured with a microscope (Olympus MVX10, Japan) equipped with a digital camera (ColorView II, Soft Imaging System, Olympus).
CFDA-SE cell proliferation assay
Cell proliferation determination was conducted by CFDA-SE probe. Briefly, cells (5 × 102) were seeded and stained with CFDA-SE in 6-well plates according to the manufacturer’s protocol. Then, cells were exposed to a series of concentrations of EVO for six days. CFDA-SE fluorescence was detected by flow cytometry (BD FACS Canto™, BD Biosciences, San Jose, USA) and calculated by FlowJo software (Treestar, Ashland, OR, USA).
Cell cycle assay
Cell cycle distribution was determined as previously described48. After the indicated treatments, cells were washed with cold PBS and harvested by centrifugation. Then, cells were re-suspended in 70% (v/v) cold ethanol and stored at −20 °C overnight. After 30-minute incubation with propidium iodide (PI) solution in the dark, cell cycle distribution was analyzed by flow cytometry (BD FACS Canto™, BD Biosciences, San Jose, USA). Results were calculated by Mod Fit LT software (version 3.0).
A2780/WT and A2780/PTXR cells were treated with different concentrations of EVO for 24 hours and the total protein was extracted with RIPA lysis buffer containing 1% phenylmethane- sulfonylfluoride (PMSF) and 1% protease inhibitor cocktail. As per our previous report48, the BCA protein assay kit (Pierce) was applied to determine protein concentrations. Equal amounts of total protein were subjected to sodium dodecyl sulfate-polyacrylamide gel electrophoresis (SDS-PAGE) and were transferred onto a polyvinylidene fluoride (PVDF) membrane. Blocking overnight was at 4 °C with 5% non-fat milk. The membrane was incubated for two hours with the primary antibodies (dilution ration 1:1000) at room temperature, including Cyclin B1, p27, p21, Rb, p-Cdc2 (Thr161), Cdc2, p-ERK (Thr202/Tyr204), ERK, p38, Ras, GAPDH and β-actin and the incubation for the secondary antibodies was one hour at room temperature. Bands visualization was conducted by an ECL Advance Western Blotting Detection Kit (Amersham, UK). The densities were calculated by the Quantity One Software (Bio-Rad, CA, USA) and were normalized by β-actin.
Dual-luciferase reporter assay
A2780/PTXR cells (1 × 104) were plated per well in a 24-well plate overnight. A2780/PTXR cells were co-transfected with 0.8 μg pRb-luc and 0.8 μg pRL-TK as a transfection efficiency control. The plasmids and TurbotFect transfection reagent were diluted in Opti-MEM reduced serum medium according to TurbotFect transfection reagent protocol. The diluted DNA was mixed together with diluted TurbotFect transfection reagent at a 1:2 ratio and incubated at 25 °C for 20 minutes. 100 μL of complexes was transferred to each well. After overnight incubation, the cells were refreshed and cultured in the completed medium for an additional 24 hours. Then, cells were exposed to a series of concentrations of EVO for 24 hours. Cell lysates were collected by passive lysis buffer and were detected using the SpectraMax M5 microplate reader. Resulting data were normalized to pRL-TK values.
siRNA-mediated RNA interference
The detailed procedure for performing target gene silencing has been described previously49. In our study, we used the Cyclin B1 siRNA: 5′-CCAAACCUUUGUAGUGAAUTT-3′ (Seq. I). We also used another siRNA sequence, 5′-GGUUGUUGCAGGAGACCAUTT -3′ (Seq. II), for silencing the Cyclin B1 gene and then investigated the Cyclin B1 expressions and cell cycle distribution. A FAM siRNA duplex with the target sequence, 5′-CGGCAAGCUGACCCUGAAGTT-3′ was employed as a non-silencing control. A2780/PTXR cells were transfected with siRNAs using Lipofectamine 2000 according to the manufacturer’s instructions (Invitrogen, Carlsbad, CA, USA). After a 4-hour transfection, the cells were cultivated in the completed medium for an additional 48 hours. Cyclin B1 siRNA-transfected or control A2780/PTXR cells (2 × 105) were co-cultured in 6-well plates. After 24 hours of EVO treatments (10 μM), cell cycle distribution was analyzed by flow cytometry (BD FACS Canto™, BD Biosciences, San Jose, USA). Results were calculated by Mod Fit LT software (version 3.0).
P-gp expression assay
P-gp expression was evaluated by the antibody P-glycoprotein conjugated FITC (BD Biosciences). A2780/WT and A2780/PTXR cells were seeded onto 6-well plates and the cells were treated with different concentrations of EVO for 24 hours. Next, cells were harvested and incubated with 100 μl P-gp antibody dye-loading buffer at 37 °C for 30 minutes protected from light. The FITC fluorescence was detected using flow cytometry (BD FACS Canto™, BD Biosciences, San Jose, USA). All experiments were performed in triplicate and compared to negative controls.
P-gp function assay
Calcium AM was used to determine the activity of P-gp. A2780/PTXR. cells were seeded onto 6-well plates and the cells were treated with different concentrations of EVO for one hour. Next, 100 μl calcium AM dye-loading solution was added to each well and incubated at 37 °C for 30 minutes protected from light. Cells were harvested and intracellular fluorescence was detected using flow cytometry (BD FACS Canto™, BD Biosciences, San Jose, USA). All experiments were performed in triplicate and compared to negative controls.
All data represent the mean of at least three separately performed experiments. The significance of variations was evaluated by GraphPad Prism software (GraphPad Software, USA). Student’s t-test was used for statistical comparison. P values less than 0.05 was considered significant.
The effect of EVO on cell viability of human epithelial ovarian cancer cells A2780/WT, A2780/PTXR and normal cell RAW 264.7
Paclitaxel-sensitive and -resistant A2780 cells were obtained and assessed by P-gp protein expression. As shown in Fig. 1A, A2780/PTXR cells were differentiated by florescence intensity from A2780/WT cells as a result of the elevated P-gp protein. Viability of the A2780/PTXR cells after PTX treatments (0.1, 1 and 10 μM) for 24 hours was assessed by MTT assay and no significant variations were observed in Fig. 1B. Those results showed that A2780/PTXR cells were resistant to paclitaxel, with an IC50 value of 550.9 μM.
As shown in Fig. 1C,D, the cytotoxicity induced by EVO in A2780/WT and A2780/PTXR cells was determined by the LDH assay. After a series of EVO (0.1, 1 and 10 μM) treatment for 24 hours, no significant variations were observed in both cell lines. Then, the cell viability after EVO treatment (0.01, 0.1, 1, 10 μM) for 24 hours in both cell lines was assessed by the MTT assay. As shown in Fig. 1E,F, 1 μM and 10 μM of EVO significantly inhibited cell viability in both cell lines. Otherwise, EVO (0 to 10 μM) exhibited no effect on RAW 264.7 cell viability after 24 hours treatment, with an IC50 value of 132.1 μM (Fig. s1A).
The effect of EVO on malignant proliferation of A2780/WT and A2780/PTXR cells
After confirming a significant variation of cell viability induced by EVO, morphology observation was conducted to visualize the influence on the proliferation of A2780/WT and A2780/PTXR cells. At concentrations of 1 μM and 10 μM, the cell population showed dramatic depletions after EVO incubation in both cell lines, with a reduction exceeding 50 percentages as shown in Fig. 2A,B. Further, in the clone formation assay, steep declines were observed after 1 μM and 10 μM EVO treatment in A2780/WT cells, as shown in Fig 3A and in Fig. 3B, almost no clones were observed after 1 μM and 10 μM EVO treatment in A2780/PTXR cells. The proliferation influence was also assessed by CFDA-SE assay through fluorescence alterations. In Fig. 4, after a series of EVO (0.01, 0.1 and 1 μM) treatment for six days, cell proliferation was assessed and 1 μM of EVO significantly suppressed cell proliferation in A2780/WT and A2780/PTXR cells. Proliferation suppression was found to be much more obvious in A2780/PTXR cells with a gradual increase, as shown in the colony formation assay.
EVO induced cell cycle arrest in dose- and time-dependent manners
Cell cycle distribution was conducted by flow cytometer analysis and a series of concentrations of EVO (0.1, 1 and 10 μM) induced G2/M phase arrest with a significance observed in A2780/WT and A2780/PTXR cells, as shown in Fig. 5. In the time courses, G2/M phase arrest was also found after different durations (0, 3, 6 and 12 hours), as shown in Fig. 6. Therefore, EVO was confirmed to induce G2/M phase arrest in a dose- and time-dependent manner in both cell lines. Moreover, EVO also significantly induced sub-G1 phase arrest in both cell lines. Those results indicated that EVO promoted apoptotic death in ovarian cancer cells.
The underlying mechanism of the anti-proliferative effect of EVO
After the EVO treatment mentioned above, the expression alterations of related proteins in A2780/WT and A2780/PTXR cells were determined by western blotting, as shown in Fig. 7. EVO up-regulated Cyclin B1, p27 and p21 in both cell lines, down-regulated Rb and inhibited Cdc2 (Thr161) phosphorylation and ERK (Thr202/Tyr204) phosphorylation in both cell lines. Furthermore, EVO decreased Ras protein and increased p38 protein expression in A2780/WT and A2780/PTXR cells. Additionally, EVO down-regulated Cdc2 expression in A2780/WT cells, but up-regulated Cdc2 expression in A2780/PTXR cells. We further investigated other alterations in CDK induced by EVO in A2780/PTXR cells. Our results showed that EVO continued to up-regulate CDK4 expression and down-regulate the protein expressions of CDK2 and CDK6 in A2780/PTXR cells (Fig. s1B).
Next, we illustrated the effect of EVO on pRb transcriptional activity in A2780/PTXR cells. Cells were transiently co-transfected with pRb-luc and pRL-TK and then treated with a series of concentrations of EVO (0.1, 1 and 10 μM). Our results showed that EVO significantly decreased pRb transcriptional activity in a dose-dependent manner (Fig. 8A). In our pre-experiments, western blotting assay confirmed that the knock-down effect of si-Cyclin B1 (Seq. II) was stronger than si-Cyclin B1 (Seq. I) (Fig. s1C and D). As a result, Cyclin B1 siRNA-transfected or control A2780/PTXR cells were co-cultured for our next experiment in 6-well plates where the high transfection efficacy was also observed (Fig. s1E). Overall, EVO was found to have different effects on multiple transfected cells (Fig. 8B) including the observation that knocking-down Cyclin B1 could attenuate the G2/M phase arrest that is induced by EVO (10 μM) in A2780/PTXR cells (Fig. 8C,D).
In A2780/PTXR cells, 1 μM and 10 μM of EVO dramatically decreased the expression level of MDR-1 evaluated by western blotting, as shown in Fig. 9A. Meanwhile, FITC-P-gp staining assay by flow cytometry showed that EVO also inhibited MDR-1 protein expression at a concentration of 1μM in A2780/PTXR cells, as shown in Fig. 9B. In the calcium AM staining assay, P-gp function evaluation was assessed further by flow cytometry, as shown in Fig. 9C. After one hour pro-treatment of EVO, 30-minute incubation with calcium AM was conducted to determine fluorescence alterations. 10 μM of EVO induced a fluorescence enhancement of calcium AM, also indicating the inhibition of P-gp function in A2780/PTXR cells.
In our present study, human epithelial ovarian cancer cells, A2780 were utilized to establish a chemo-resistant cell line through stepwise concentration exposure, in order to investigate the chemo-resistance influence of an active constituent from Chinese medicine. The resistance to PTX was also confirmed by a lack of obvious variation of cell viability through the MTT assay in A2780/PTXR cells. The effect of EVO on cell viability of human epithelial ovarian cancer cells, A2780/WT and A2780/PTXR was conducted through the MTT assay. Remarkable inhibitions on cell viability such as the high concentrations (1 μM and 10 μM) were much more pronounced than the low concentrations (0.01 μM and 0.1 μM) and were observed in both A2780/WT and A2780/PTXR cells. Notably, this is the first time that the effects of EVO on human epithelial ovarian cancer and resistant human epithelial ovarian cancer have been investigated. Although there have been intensive reports on a variety of cancer types, this is the first time that the proliferation inhibition in epithelial ovarian cancer cells, A2780/WT and the related chemo-resistant cell A2780/PTXR has been confirmed.
In this experiment, no significant alterations of the LDH release levels have been observed which would indicate that EVO induced cell viability inhibition but caused no cytotoxic effect. EVO also exhibited no cytotoxic effect on RAW 264.7 cells even at 10 μM. These findings suggested that EVO maintains certain selectivity to cancer cells. To verify, the morphology of the cell number change was visualized and representative images of colony formation also confirmed the decreased growth rates of both cell lines. The proliferation influence of EVO was also confirmed by CFDA-SE assay through fluorescence alterations. Overall, the potential anti-proliferative effect of EVO might be induced through cell cycle arrest at the G2/M phase and the sub-G1 phase.
The cyclin-dependent kinases (CDKs), specifically CDK1, CDK2, CDK4 and CDK6 play an important role in regulating cell cycle50. The activation of CDK1 (Cdc2), which is close to G2/M phase cell cycle arrest, promotes mitosis in cell cycle progression, which requires cyclin binding and phosphosrylation activation at Thr161. Meanwhile, EVO inhibits Cdc2 phosphorylation at Thr161. Therefore, the activation failure of Cdc2 still occupies the main position after EVO treatment. This activation failure might be consistent with the induced cell cycle arrest at the G2/M phase. Moreover, EVO down-regulated Cdc2 expression in A2780/WT cells, but up-regulated Cdc2 expression in A2780/PTXR cells. It has been reported that inhibition of certain cell cycle CDKs may be compensated for by other CDKs51, thus additional CDKs alterations induced by EVO were further investigated in A2780/PTXR cells. Our results suggested that EVO inhibition on the protein expressions of CDK2 and CDK6 could be compensated for by Cdc2 and CDK4 in A2780/PTXR cells.
In our present study, the increase of Cyclin B1 induced by EVO was observed robustly in both A2780/WT and A2780/PTXR cells. This was also the first time that EVO increased the expression level of Cyclin B1 in human epithelial ovarian cancer, A2780 and the related PTX-resistant cell lines. Although Cyclin B1 was always over-expressed and led to uncontrolled growth in many cancer cell lines, when in reference to human ovarian cancer cells, there were a few controversial reports. For instance, besides the suppression of Cyclin B1 expression52,53,54,55, there was also a Cyclin B1 increase in correspondence with the S-phase arrest induced by taxol and cisplatin in cisplatin-resistant A2780 cells56. There was also an up-regulation of Cyclin B1 in ovarian cancer cells, A2780-1A9 that was observed while overcoming multidrug resistance57. Therefore, the activation failure of Cdc2 might be attributed to an overall expression of other unknown activating factors and might require further investigation.
p27 and p21 are regarded as tumor suppressors involved in regulating cell cycle progression. The up-regulated expressions of p27 and p21 induced by EVO in both A2780/WT and A2780/PTXR cells also indicate activation failure of Cdc2. The inactivation of Rb cooperated with cyclin-dependent kinase activation in order to promote cell division and proliferation. Although Rb suppression by EVO might likely contribute to cell cycle progression, the activation failure or inhibition of Cdc2 mentioned above would also determine the eventual commitment of cell cycle arrest. Actually, reports showed that tumor development was regulated by the cooperation of p27 and Rb through integrating regulatory signals. As the main factors in the MAPK pathway, ERK1/2 phosphorylation and p38 expression showed different responses after EVO treatments, remarkable inhibition and increased alteration, respectively. The significant inhibition of ERK1/2 phosphorylation was consistent with the anti-proliferative effect of EVO. The over-expressed Ras was closely related to the MAPK signaling pathway and the decreased level induced by EVO indicated an enhancing anti-proliferative potential in human epithelial ovarian cancer, A2780 and the related PTX-resistant cell lines. Besides, the expression level of MDR-1 was reduced after EVO treatment in A2780/PTXR cells. Those results were confirmed by both western blotting and flow cytometry. A fluorescence enhancement of calcium AM gave further testimony to MDR-1 function inhibition by EVO in chemo-resistance.
In our present study, EVO was observed to have significant proliferation suppression for the first time in human epithelial ovarian cancer cells, A2780 and the related PTX-resistant cell line. The declined clone formation and representative fluorescence of CFDA-SE both confirmed this inhibition of malignant proliferation. Meanwhile, EVO induced cell cycle arrest in a dose- and time-dependent manner, as confirmed by FACs assay. This cell division disturbance might be mediated by the cooperation of Cyclin B1 and Cdc2, including the up-regulation of Cyclin B1, p27, p21 and activation failure of Cdc2. The regulation of the MAPK signaling pathway also assisted in this process. Furthermore, EVO significantly decreased pRb transcriptional activity and knocking-down Cyclin B1 could attenuate the G2/M phase arrest induced by EVO (10 μM) in A2780/PTXR cells. Our results indicated that EVO suppressed cell proliferation through G2/M phase cell cycle arrest via regulation of the Rb and Cyclin B1 signaling pathways. EVO also indicated an enhancing chemo-sensitivity potential in A2780/PTXR cells, through down-regulating the expression level of MDR-1 accompanied with MDR-1 function suppression.
Taken together, we confirmed that EVO exerted an anti-proliferative effect on human epithelial ovarian cancer cells and resistant human epithelial ovarian cancer cells, through inducing cell cycle arrest at the G2/M phase. It was also involved in Cyclin B1/Cdc2, p27/Rb, MAPK signaling pathways and it improved chemo-resistance partly by contributing to the suppression of P-gp protein expression and function. Overall, we found that EVO significantly suppressed malignant proliferation in human epithelial ovarian cancer, thus proving to be a potential anti-cancer agent in the future.
How to cite this article: Zhong, Z.-F. et al. Anti-proliferative activity and cell cycle arrest induced by evodiamine on paclitaxel-sensitive and -resistant human ovarian cancer cells. Sci. Rep. 5, 16415; doi: 10.1038/srep16415 (2015).
Li, J. et al. Apoptosis and chemoresistance in human ovarian cancer: is Xiap a determinant? Biological signals and receptors 9, 122–130 (2000).
Cheng, J. Q. et al. Role of X-linked inhibitor of apoptosis protein in chemoresistance in ovarian cancer: possible involvement of the phosphoinositide-3 kinase/Akt pathway. Drug resistance updates 5, 131–146 (2002).
Ali, A. Y. et al. Molecular determinants of ovarian cancer chemoresistance: new insights into an old conundrum. Annals of the New York Academy of Sciences 1271, 58–67 (2012).
Wang, W. & Figg, W. D. Secondary BRCA1 and BRCA2 alterations and acquired chemoresistance. Cancer biology & therapy 7, 1004–1005 (2008).
Ahmed, N., Abubaker, K., Findlay, J. & Quinn, M. Epithelial mesenchymal transition and cancer stem cell-like phenotypes facilitate chemoresistance in recurrent ovarian cancer. Current cancer drug targets 10, 268–278 (2010).
Ahmed, N., Abubaker, K., Findlay, J. & Quinn, M. Cancerous ovarian stem cells: obscure targets for therapy but relevant to chemoresistance. Journal of cellular biochemistry 114, 21–34 (2013).
Suh, D. H., Kim, M. K., No, J. H., Chung, H. H. & Song, Y. S. Metabolic approaches to overcoming chemoresistance in ovarian cancer. Annals of the New York Academy of Sciences 1229, 53–60 (2011).
Suh, D. H., Kim, M. K., Kim, H. S., Chung, H. H. & Song, Y. S. Epigenetic therapies as a promising strategy for overcoming chemoresistance in epithelial ovarian cancer. Journal of cancer prevention 18, 227–234 (2013).
Zhou, J., O’Brate, A., Zelnak, A. & Giannakakou, P. Survivin deregulation in β-tubulin mutant ovarian cancer cells underlies their compromised mitotic response to taxol. Cancer research 64, 8708–8714 (2004).
Chabalier, C. et al. BRCA1 downregulation leads to premature inactivation of spindle checkpoint and confers paclitaxel resistance. Cell cycle 5, 1001–1007 (2006).
Rivera, A., Mavila, A., Bayless, K. J., Davis, G. E. & Maxwell, S. A. Cyclin A1 is a p53-induced gene that mediates apoptosis, G2/M arrest and mitotic catastrophe in renal, ovarian and lung carcinoma cells. Cellular and molecular life sciences 63, 1425–1439 (2006).
Bansal, N. et al. BCL2 antagonist of cell death kinases, phosphatases and ovarian cancer sensitivity to cisplatin. Journal of gynecologic oncology 23, 35–42 (2012).
Yan, F., Shao, L. J. & Hu, X. Y. Knockdown of UHRF1 by lentivirus-mediated shRNA inhibits ovarian cancer cell growth. Asian Pacific journal of cancer prevention 16, 1343–1348 (2015).
Innocente, S. A., Abrahamson, J. L., Cogswell, J. P. & Lee, J. M. p53 regulates a G2 checkpoint through cyclin B1. Proceedings of the National Academy of Sciences of the United States of America 96, 2147–2152 (1999).
Zheng, H. et al. Nuclear cyclin B1 is overexpressed in low-malignant-potential ovarian tumors but not in epithelial ovarian cancer. American journal of obstetrics and gynecology 201, 367 e361-366 (2009).
Seviour, E. G. et al. Functional proteomics identifies miRNAs to target a p27/Myc/phospho-Rb signature in breast and ovarian cancer. Oncogene 10.1038/onc.2014.469 (2015).
Liu, Z. et al. miR-106a represses the Rb tumor suppressor p130 to regulate cellular proliferation and differentiation in high-grade serous ovarian carcinoma. Molecular cancer research 11, 1314–1325 (2013).
Corney, D. C., Flesken-Nikitin, A., Choi, J. & Nikitin, A. Y. Role of p53 and Rb in ovarian cancer. Advances in experimental medicine and biology 622, 99–117 (2008).
Emmanuel, C. et al. Genomic classification of serous ovarian cancer with adjacent borderline differentiates RAS pathway and TP53-mutant tumors and identifies NRAS as an oncogenic driver. Clinical cancer research 20, 6618–6630 (2014).
Sheppard, K. E. et al. Synergistic inhibition of ovarian cancer cell growth by combining selective PI3K/mTOR and RAS/ERK pathway inhibitors. European journal of cancer 49, 3936–3944 (2013).
Sedlakova, I. et al. Clinical significance of the resistance proteins LRP, Pgp, MRP1, MRP3 and MRP5 in epithelial ovarian cancer. International journal of gynecological cancer 25, 236–243 (2015).
Zou, Y. et al. Apoptosis of human non-small-cell lung cancer A549 cells triggered by evodiamine through MTDH-dependent signaling pathway. Tumour biology 36, 5187–5193 (2015).
Bai, X., Meng, H., Ma, L. & Guo, A. Inhibitory effects of evodiamine on human osteosarcoma cell proliferation and apoptosis. Oncology letters 9, 801–805 (2015).
Fang, C. et al. Evodiamine induces G2/M arrest and apoptosis via mitochondrial and endoplasmic reticulum pathways in H446 and H1688 human small-cell lung cancer cells. PloS one 9, e115204 (2014).
Hong, J. Y., Park, S. H., Min, H. Y., Park, H. J. & Lee, S. K. Anti-proliferative effects of evodiamine in human lung cancer cells. Journal of cancer prevention 19, 7–13 (2014).
Khan, M., Bi, Y., Qazi, J. I., Fan, L. & Gao, H. Evodiamine sensitizes U87 glioblastoma cells to TRAIL via the death receptor pathway. Molecular medicine reports 11, 257–262 (2015).
Chien, C. C. et al. Activation of JNK contributes to evodiamine-induced apoptosis and G2/M arrest in human colorectal carcinoma cells: a structure-activity study of evodiamine. PloS one 9, e99729 (2014).
Wang, S. et al. Evodiamine synergizes with doxorubicin in the treatment of chemoresistant human breast cancer without inhibiting P-glycoprotein. PloS one 9, e97512 (2014).
Zhang, T., Qu, S., Shi, Q., He, D. & Jin, X. Evodiamine induces apoptosis and enhances TRAIL-induced apoptosis in human bladder cancer cells through mTOR/S6K1-mediated downregulation of Mcl-1. International journal of molecular sciences 15, 3154–3171 (2014).
Yang, L. et al. Growth inhibition and induction of apoptosis in SGC7901 human gastric cancer cells by evodiamine. Molecular medicine reports 9, 1147–1152 (2014).
Wang, K. L. et al. Anti-proliferative effects of evodiamine on human breast cancer cells. PloS one 8, e67297 (2013).
Yang, J. et al. Evodiamine inhibits STAT3 signaling by inducing phosphatase shatterproof 1 in hepatocellular carcinoma cells. Cancer letters 328, 243–251 (2013).
Rasul, A. et al. Cytotoxic effect of evodiamine in SGC-7901 human gastric adenocarcinoma cells via simultaneous induction of apoptosis and autophagy. Oncology reports 27, 1481–1487 (2012).
Wei, W. T. et al. Enhanced antitumor efficacy of gemcitabine by evodiamine on pancreatic cancer via regulating PI3K/Akt pathway. International journal of biological sciences 8, 1–14 (2012).
Huang, H. et al. Acid sphingomyelinase contributes to evodiamine-induced apoptosis in human gastric cancer SGC-7901 cells. DNA and cell biology 30, 407–412 (2011).
Chen, M. C. et al. Anti-proliferative effects of evodiamine on human thyroid cancer cell line ARO. Journal of cellular biochemistry 110, 1495–1503 (2010).
Wang, X. N. et al. Enhancement of apoptosis of human hepatocellular carcinoma SMMC-7721 cells through synergy of berberine and evodiamine. Phytomedicine 15, 1062–1068 (2008).
Yang, J., Wu, L. J., Tashino, S., Onodera, S. & Ikejima, T. Reactive oxygen species and nitric oxide regulate mitochondria-dependent apoptosis and autophagy in evodiamine-treated human cervix carcinoma HeLa cells. Free radical research 42, 492–504 (2008).
Kan, S. F. et al. Anti-proliferative effects of evodiamine on human prostate cancer cell lines DU145 and PC3. Journal of cellular biochemistry 101, 44–56 (2007).
Huang, D. M. et al. Induction of mitotic arrest and apoptosis in human prostate cancer pc-3 cells by evodiamine. The Journal of urology 173, 256–261 (2005).
Kan, S. F., Huang, W. J., Lin, L. C. & Wang, P. S. Inhibitory effects of evodiamine on the growth of human prostate cancer cell line LNCaP. International journal of cancer 110, 641–651 (2004).
Huang, Y. C., Guh, J. H. & Teng, C. M. Induction of mitotic arrest and apoptosis by evodiamine in human leukemic T-lymphocytes. Life sciences 75, 35–49 (2004).
Fei, X. F. et al. Evodiamine, a constituent of Evodiae Fructus, induces anti-proliferating effects in tumor cells. Cancer science 94, 92–98 (2003).
Ogasawara, M., Matsubara, T. & Suzuki, H. Screening of natural compounds for inhibitory activity on colon cancer cell migration. Biological & pharmaceutical bulletin 24, 720–723 (2001).
Li, Z. et al. MiR-27a modulates MDR1/P-glycoprotein expression by targeting HIPK2 in human ovarian cancer cells. Gynecologic oncology 119, 125–130 (2010).
Zahedifard, M. et al. Synthesis, characterization and apoptotic activity of quinazolinone Schiff base derivatives toward MCF-7 cells via intrinsic and extrinsic apoptosis pathways. Scientific Reports 5, 11544 (2015).
Zhong, Z. et al. Furanodiene, a natural product, inhibits breast cancer growth both in vitro and in vivo. Cellular physiology and biochemistry 30, 778–790 (2012).
Zhong, Z., Tan, W., Chen, X. & Wang, Y. Furanodiene, a natural small molecule suppresses metastatic breast cancer cell migration and invasion in vitro. European journal of pharmacology 737, 1–10 (2014).
Liang, L. et al. Dihydroquercetin (DHQ) induced HO-1 and NQO1 expression against oxidative stress through the Nrf2-dependent antioxidant pathway. Journal of agricultural and food chemistry 61, 2755–2761 (2013).
Enders, G. H. Mammalian interphase cdks: dispensable master regulators of the cell cycle. Genes & cancer 3, 614–618 (2012).
Ali, S. et al. The development of a selective cyclin-dependent kinase inhibitor that shows antitumor activity. Cancer research 69, 6208–6215 (2009).
Bodo, J. et al. Sensitisation for cisplatin-induced apoptosis by isothiocyanate E-4IB leads to signalling pathways alterations. British journal of cancer 95, 1348–1353 (2006).
Lee, R. X., Li, Q. Q. & Reed, E. β-elemene effectively suppresses the growth and survival of both platinum-sensitive and -resistant ovarian tumor cells. Anticancer research 32, 3103–3113 (2012).
Li, B. et al. Chaetoglobosin K induces apoptosis and G2 cell cycle arrest through p53-dependent pathway in cisplatin-resistant ovarian cancer cells. Cancer letters 356, 418–433 (2015).
Li, X. et al. Valeriana jatamansi constituent IVHD-valtrate as a novel therapeutic agent to human ovarian cancer: in vitro and in vivo activities and mechanisms. Current cancer drug targets 13, 472–483 (2013).
Zaffaroni, N. et al. Induction of apoptosis by taxol and cisplatin and effect on cell cycle-related proteins in cisplatin-sensitive and -resistant human ovarian cells. British journal of cancer 77, 1378–1385 (1998).
Du, J. et al. Evodiamine induces apoptosis and inhibits metastasis in MDAMB-231 human breast cancer cells in vitro and in vivo. Oncology reports 30, 685–694 (2013).
This study was supported by the Macao Science and Technology Development Fund (077/2011/A3 and 048/2013/A2) and the Research Fund of University of Macau (CPG2014-00012-ICMS, UL016/09Y4/CMS/WYT01/ICMS and MYRG208 (Y3-L4)-ICMS11-WYT). W.A. Qiang was partially supported by the Baskes Foundation and Robert H. Lurie Comprehensive Cancer Center at the Northwestern University. We also thank Stacy Ann Kujawa in Northwestern University Feinberg School of Medicine for critical proofreading of the manuscript.
The authors declare no competing financial interests.
Electronic supplementary material
About this article
Cite this article
Zhong, ZF., Tan, W., Wang, SP. et al. Anti-proliferative activity and cell cycle arrest induced by evodiamine on paclitaxel-sensitive and -resistant human ovarian cancer cells. Sci Rep 5, 16415 (2015). https://doi.org/10.1038/srep16415
BMC Complementary Medicine and Therapies (2020)
Evodiamine in combination with histone deacetylase inhibitors has synergistic cytotoxicity in thyroid carcinoma cells
Chinese Medicine (2018)
The in vitro estrogenic activity of the crude drugs found in Japanese herbal medicines prescribed for menopausal syndrome was enhanced by combining them
BMC Complementary and Alternative Medicine (2018)
Journal of Natural Medicines (2018)