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. 2016 Aug 2;36(4):1799–1806. doi: 10.3892/or.2016.4992

Schisandrin B inhibits cell proliferation and induces apoptosis in human cholangiocarcinoma cells

Xiaohui Yang 1, Shuai Wang 1, Yunchuan Mu 1, Yixiong Zheng 2,✉
PMCID: PMC5022873  PMID: 27499090

Abstract

Cholangiocarcinoma (CCA) is the second most common hepatic cancer with high resistance to current chemotherapies and extremely poor prognosis. The present study aimed to examine the effects of schisandrin B (Sch B) on CCA cells both in vitro and in vivo and to examine its underlying mechanism. We found that Sch B inhibited the viability and proliferation of CCA cells in a dose- and time-dependent manner as assessed by MTT and colony formation assays. The flow cytometric assay revealed G0/G1 phase arrest in the Sch B-treated HCCC-9810 and RBE cells. In addition, Sch B induced intrahepatic cholangiocarcinoma apoptosis as shown by the results of Annexin V/PI double staining. Rhodamine 123 staining revealed that Sch B decreased the mitochondrial membrane potential (ΔΨm) in a dose-dependent manner. Mechanistically, western blot analysis indicated that Sch B induced apoptosis by upregulating Bax, cleaved caspase-3, cleaved caspase-9 and cleaved PARP, and by downregulating cyclin D1, Bcl-2 and CDK-4. Moreover, Sch B significantly inhibited HCCC-9810 xenograft growth in athymic nude mice. In summary, these findings suggest that Sch B exhibited potent antitumor activities via the induction of CCA apoptosis and that Sch B may be a promising drug for the treatment of CCA.

Keywords: schisandrin B, cholangiocarcinoma, proliferation, apoptosis, cell cycle

Introduction

Cholangiocarcinoma (CCA) is a highly malignant adenocarcinoma that originates in the extrahepatic and liver bile ducts, which terminate at the ampulla of Vater (1). CCA is generally classified into 3 forms: intrahepatic cholangiocarcinoma (ICC), hilar cholangiocarcinoma and extrahepatic cholangiocarcinoma (ECC) (2). Although CCA is a relatively rare neoplasm with an annual incidence rate of 1–2 cases/100,000 in the Western world, the overall incidence and mortality rates of this neoplasm appear to be rising worldwide over the past several decades (3,4). Due to its late clinical presentation and the lack of effective non-surgical therapeutic modalities, the disease is difficult to diagnose and is frequently fatal (5). Over the past 30 years, the overall 5-year survival rate for patients with CCA, including those who have undergone resection, is less than 10% (6). Moreover, high drug resistance usually lowers the efficacy of chemotherapy drugs (7). Therefore, novel effective strategies and drugs are urgently needed to improve outcomes for patients with CCA.

For centuries, schisandrin B (Sch B; Fig. 1) has been a major traditional Chinese medicine. Sch B is extracted from the fruit of Schisandra chinensis Baill., and has been used to treat several human diseases, including hepatitis and myocardial disorders (8). In addition, more studies have increasingly shown that Sch B possesses antitumor activity in various types of human cancers, including glioma, gastric and breast cancer, and hepatoma (9–12). Previous studies have shown that Sch B attenuates cancer invasion and metastasis with very low toxicity (13), and it inactivates ATR when DNA damage occurs (14). However, to the best of our knowledge, the effects of Sch B on CCA cells and the underlying mechanisms of these effects have not been previously reported. In the present study, we investigated the anticancer effects of Sch B on human CCA cell lines (HCCC-9810 and RBE) and the possible molecular mechanisms underlying these actions, which provided experimental evidence for the potential application of Sch B as a new natural antitumor medicine for CCA.

Figure 1.

Figure 1

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Chemical structure of schisandrin B.

Materials and methods

Cell lines and culture

The human CCA HCCC-9810 and RBE cell lines were purchased from the Shanghai Institute of Cell Biology, Chinese Academy of Sciences (CAS; Shanghai, China). All cells were grown in RPMI-1640 medium supplemented with 10% fetal bovine serum (FBS) (both from Gibco, Grand Island, NY, USA), 100 µg/ml streptomycin and 100 U/ml penicillin (HyClone, Logan, UT, USA). The cells were then stored in a 5% CO2 atmosphere at 37°C. After reaching 80% confluency, the cells were digested with 0.25% pancreatin-ethylene diamine tetraacetic acid diluted in a ratio of 1:3.

Drugs and antibodies

Sch B and Rhodamine 123 (Rho 123) were purchased from Sigma-Aldrich (St. Louis, MO, USA). Sch B was dissolved in dimethyl sulfoxide (DMSO; Sigma-Aldrich) to create a 100 mM stock solution. The stock solution was further diluted with culture media to acquire the desired concentrations. The control groups were treated with equal volumes of DMSO. Cell Counting Kit-8 (CCK-8) was purchased from Dojindo Laboratories (Tokyo, Japan). The Annexin V/PI apoptosis kit was obtained from BD Biosciences (San Diego, CA, USA). Primary antibodies against cleaved PARP, cleaved caspase-3, CDK4, Bcl-2, Bax, cleaved caspase-9 and cyclin D1, and secondary antibodies (goat anti-rabbit) were all purchased from Cell Signaling Technology (Danvers, MA, USA). β-actin was purchased from Abways Technology (Shanghai, China).

Colony formation assay

HCCC-9810 and RBE cells were suspended in RPMI-1640 medium at a final concentration of 200 cells/ml and seeded onto 6-well plates (Corning, Corning, NY, USA). Mediim containing 10% FBS was replaced every 3 days. The cells were fixed and stained when a signal colony contained >50 cells. Then, colony-forming units were microscopically photographed. The results are expressed as the average of 3 independent experiments.

Cell viability assay

Cells were diluted into single cell suspensions and seeded in 96-well plates (1×103 cells/well) in 100 µl culture medium. Following overnight incubation, the cells were treated with various concentrations (0, 10, 20, 40, 80 and 160 µmol/l) of Sch B. At each time point (24, 48 and 72 h), 10 µl CCK-8 solution was added to each well and incubated for 3 h in the incubator, and the absorbance was determined at 450 nm using a microplate reader (Bio-Tek, Winooski, VT, USA). The cell survival rate was calculated as the percentage of absorbance in individual Sch B-treated wells vs. untreated control wells. The results represent the average of 5 parallel samples. All experiments were repeated at least 3 times.

Cell cycle analysis

After treatment with different concentrations of Sch B for 48 h, HCCC-9810 and RBE cells were harvested, fixed in 70% ethanol and stored at 4°C. On the day of analysis, the cells were washed and incubated in staining buffer [10 mg/ml RNase and 1 mg/ml propidium iodide (PI) (Sigma-Aldrich)] at 37°C in the dark for 30 min. Next, the samples were analyzed using flow cytometry (BD Biosciences). Cell Quest acquisition software was used to calculate the percentages of cells in the G0/G1, S and G2/M phases.

Mitochondrial membrane potential (ΔΨm) assay

Rho 123 was used to measure the ΔΨm according to previously reported methods with some modifications (15). Briefly, after treatment with Sch B (20, 40 and 80 µmol/l) for 48 h, cells were harvested and incubated with medium containing Rho 123 (10 µg/ml) for 30 min in a 5% CO2 atmosphere at 37°C in the dark. The samples were then analyzed by flow cytometry. In all cases, the samples were gated to exclude cellular debris. Each assay was carried out in triplicate, and the results are expressed as the mean ± SD.

Cell apoptosis assay

Apoptosis was detected using the FITC Annexin V apoptosis detection kit (BD Biosciences) according to the manufacturer's instructions. Briefly, cells were treated with Sch B (0, 20, 40 and 80 µmol/l) for 48 h. The cells were then washed and resuspended in 1X binding buffer at a density of 1×106 cells/ml. Then, the cells were incubated with 5 µl Annexin V-FITC and 5 µl PI (100 µg/ml) for 15 min in the dark at room temperature. The stained cells were diluted with 400 µl binding buffer and immediately detected by flow cytometry (BD Biosciences). Each sample was assayed in duplicate, and the experiment was repeated 3 times.

Western blot analysis

HCCC-9810 and RBE cells were treated with Sch B (0, 20, 40 and 80 µmol/l) for 48 h. The cells were harvested and lysed in RIPA buffer (Beyotime Institute of Biotechnology, Beijing, China) supplemented with protease inhibitor (Roche Applied Science, Indianapolis, IN, USA) at 4°C for 15 min. Then, cells were centrifuged in a microcentrifuge at 12,000 × g for 15 min at 4°C to collect the supernatant. The protein concentration was measured using the bicinchoninic acid (BCA) assay kit (Beyotime). A total of 30 µg of protein/lane was subjected to SDS-polyacrylamide gel electrophoresis (PAGE) after boiling for 5 min in 1X SDS sample buffer, and then electrophoretically transferred to polyvinylidene difluoride membranes (Millipore, Bedford, MA, USA). After blocking with 5% skim milk for 1–2 h at room temperature, the membranes were then incubated with the indicated primary antibodies against Bcl-2, Bax, cleaved caspase-9, cleaved PARP, cyclin D1, cleaved caspase-3, CDK4 and β-actin (1:1,000) at 4°C overnight. After washing with Tris-buffered saline and Tween-20 (TBST) buffer for 3×5 min, the blots were then re-probed with the secondary antibodies conjugated to horseradish peroxidase for 1 h at room temperature. The protein bands were detected using enhanced chemiluminescence and visualized using a Gel Doc 2000 (Bio-Rad, Hercules, CA, USA).

In vivo tumor xenograft study

Male athymic nude mice (5–6 weeks old) were purchased from Shanghai SLAC Laboratory Animal Co., Ltd. (Shanghai, China). All animal experiments were performed in strict accordance with the Institutional Animal Care and Use Committee-approved protocol. The mice were housed in a specific pathogen-free environment. HCCC-9810 cells in log-phase growth (2.5×106) suspended in 100 µl phosphate-buffered saline (PBS) were subcutaneously inoculated into the right flank of the nude mice. Sch B treatment was started 7 days after inoculation of the cells. The control group (n=8) was administered PBS intraperitoneally, whereas the other two treatment groups (n=8) were administered Sch B (20 and 80 mg/kg) intraperitoneally every 2 days for up to 30 days. On day 30, all mice were sacrificed, and the tumors were removed and weighed.

Statistical analysis

All of the experiments were independently repeated 3 times. Numerical data are presented as the mean ± standard deviation. Statistically significant differences between samples were determined using the Student's t-test. P<0.05 was considered to indicate a statistically significant result.

Results

Sch B inhibits the proliferation and decreases the cell viability of CCA cells in a dose-dependent manner

To investigate the effect of Sch B on human CCA cells, HCCC-9810 and RBE cells were treated with Sch B at concentrations of 0–160 µM for 24, 48 and 72 h followed by detection of cell viability. The results of the CCK-8 assay showed that Sch B decreased the cell viability of the HCCC-9810 and RBE cells in a dose- and time-dependent manner (Fig. 2A). The IC50 values (the drug concentration that inhibited 50% of the cells) of Sch B in the HCCC-9810 and RBE cells at 48 h were 40±1.6 and 70±2.6 µmol/l, respectively. As shown in Fig. 2B and C, the numbers of colonies of RBE and HCC-9810 cells were significantly reduced in a concentration-dependent manner after treatment with Sch B. The individual colony size in Sch B-treated group was also smaller than that of control group as shown in Fig. 2B. These results suggested that Sch B inhibited the proliferation of CCA cells.

Figure 2.

Figure 2

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Schisandrin B inhibits the proliferation of CCA cells. (A) RBE and HCCC-9810 cells were treated with various concentrations of Sch B for 24, 48 and 72 h. Cell viability was examined using the CCK-8 assay. (B and C) RBE and HCCC-9810 cells were treated with Sch B (2, 4 and 8 µmol/l) for 48 h. Then, the medium was replaced with fresh medium, and the cells were cultured for another 14 days. (B) The colonies were then stained by Giemsa. (C) The numbers of colonies of RBE and HCCC-9810 cells were counted. The data are expressed as the mean ± SD of 3 replicate experiments; *P<0.05, **P<0.01, ***P<0.001 vs. the control group.

Sch B induces G0/G1 phase arrest in HCCC-9810 and RBE cells

To determine whether Sch B-induced cytotoxicity was caused by cell cycle arrest, we performed cell cycle distribution analysis in the HCCC-9810 and RBE cells after exposure to Sch B. As shown in Fig. 3A and B, Sch B induced G0/G1 phase arrest (from 82.94 to 95.75% for HCCC-9810 cells and from 81.9 to 96.62% for RBE cells) with a slight S phase decrease compared with that of the control cells.

Figure 3.

Figure 3

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Schisandrin B induces cell cycle arrest in CCA cells. (A) The cell cycle distribution of RBE and HCCC-9810 cells was evaluated by flow cytometry after the addition of different concentrations of Sch B (0, 20, 40 and 80 µmol/l) for 48 h. (B) Data are calculated and expressed as the mean ± SD (n=3). (C) Expression levels of cyclin D1 and CDK4 in RBE and HCCC-9810 cells were measured by western blot analysis with β-actin as a loading control.

Next, we assessed the protein expression of the G0/G1 phase regulatory genes after Sch B treatment. As shown in Fig. 3C, the expression levels of cyclin D1 and CDK4 were reduced in a dose-dependent manner after treatment with Sch B. These results illustrated that Sch B blocked the cell cycle to inhibit CCA cell proliferation.

Sch B induces apoptosis in human CCA cells

To further elucidate whether the inhibition of cell growth was caused by apoptosis, we performed Annexin V/PI dual staining followed by flow cytometric analysis after stimulation with various doses of Sch B. The translocation of phosphatidylserine (PS) from the inner leaflet to the outer leaflet of the plasma membrane is a marker of apoptosis. Apoptotic and necrotic cells can be identified via fluorophore-labeled Annexin V, which has a high affinity for PS. In addition, PI nucleic acid dye gains entry into late apoptotic and necrotic cells, but not into early apoptotic and living cells. Therefore, various cell populations can be easily distinguished using Annexin V/PI staining. As assessed by flow cytometry and as shown in Fig. 4A and B, the number of surviving cells was decreased (from 90.1 to 33.2% for HCCC-9810 cells and from 89.4 to 28.9% for RBE cells) and the number of early apoptotic cells was markedly increased (from 5.9 to 61.2% for HCCC-9810 cells and from 4.8 to 65.4% for RBE cells) in a dose-dependent manner after Sch B treatment compared with the control group. These results are consistent with the cell viability results as determined by the CCK-8 assay, suggesting that the apoptotic cell death pathway may play a key role in the antiproliferative effect of Sch B on HCCC-9810 and RBE cells.

Figure 4.

Figure 4

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Schisandrin B induces apoptosis in CCA cells. HCCC-9810 and RBE cells were treated with Sch B (0, 20, 40 and 80 µmol/l) for 48 h. (A) Flow cytometric analysis of apoptosis quantification by dual Annexin V-FITC and propidium iodide (PI) staining in untreated cells or Sch B-treated cells. (B) Percentages of surviving and early and late apoptotic cells are presented as the means ± SD (n=3). Significant differences from control experiments; *P<0.01, **P<0.001.

Sch B decreases ΔΨm in CCA cells

To examine whether mitochondrial membrane integrity is disrupted by Sch B treatment, cells were stained with Rho 123, and staining was detected by flow cytometry. The loss of the ΔΨm was reflected by a decrease in the intensity of Rho 123 fluorescent staining. Compared with the control cells, Sch B treatment markedly decreased Rho 123-positive cells (from 96.9 to 18.2% for HCCC-9810 cells and from 95.6 to 20.5% for RBE cells) in a dose-dependent manner (Fig. 5A and B). These findings suggest that Sch B promotes the apoptosis of CCA cells through a mitochondrial-dependent apoptotic pathway.

Figure 5.

Figure 5

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Schisandrin B disrupts mitochondrial integrity in CCA cells. HCCC-9810 and RBE cells were exposed to Sch B (0, 25, 50 and 100 µmol/l) for 48 h. (A) Rhodamine 123 staining was analyzed by flow cytometric analysis. (B) The corresponding histogram shows the percentages of cells with high ΔΨm (survival). The results shown are representative data from 3 independent experiments; *P<0.05, **P<0.01 vs. the control group.

Sch B induces apoptosis via the regulation of caspase-3 and Bcl-2 family members in CCA cells

To investigate the underlying molecular mechanisms responsible for Sch B-induced apoptosis of HCCC-9810 and RBE cells, we assessed the expression of apoptosis-related factors (cleaved PARP, Bax, Bcl-2, cleaved caspase-3 and cleaved caspase-9) after Sch B treatment by western blot analysis. As shown in Fig. 6A, increased expression of cleaved PARP, Bax, cleaved caspase-9 and cleaved caspase-3, and decreased expression of Bcl-2 was observed after Sch B treatment, which was consistent with apoptosis induced by Sch B. Furthermore, compared with the control group, the Bcl-2 (anti-apoptotic) to Bax (pro-apoptotic) ratio was significantly decreased (Fig. 6B). Our results suggest that Sch B promotes apoptosis through the regulation and activation of apoptosis-related proteins in CCA cells.

Figure 6.

Figure 6

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Schisandrin B regulates the expression of apoptosis-related proteins in CCA cells. HCCC-9810 and RBE cells were treated with Sch B for 48 h, and cell lysates were prepared. (A) The expression levels of cleaved PARP, cleaved caspase-3, cleaved caspase-9, Bax and Bcl-2 were detected by western blotting. β-actin served as a loading control. (B) The band density was determined, and the ratio of Bcl-2 to Bax was calculated. The results are expressed as the mean ± SD compared with the control (designated as 1.00); *P<0.05, **P<0.01 compared with the control group.

Sch B inhibits tumor growth in vivo

The anticancer effect of Sch B on tumor growth in vivo was further analyzed by intraperitoneally injecting vehicle (PBS) or Sch B (20 and 80 mg/kg) into nude mice bearing subcutaneous HCCC-9810 tumor xenografts every 2 days for up to 30 days. As shown in Fig. 7A and B, there was a marked dose-dependent reduction in tumor weight in mice treated with oridonin compared with the control mice.

Figure 7.

Figure 7

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Schisandrin B suppressed the growth of HCCC-9810 cells in vivo. HCCC-9810 cells were subcutaneously injected into the right flank of nude mice. Then, vehicle (PBS) or Sch B (20 and 80 mg/kg) were intraperitoneally injected every 2 days for up to 30 days. (A) At the end of the experiment, mice were sacrificed, and tumors were resected and weighed in each group. (B) A representative mouse from each group (n=6) is photographed; *P<0.05, **P<0.01, ***P<0.001 vs. the control group.

Discussion

Previous studies have demonstrated that Sch B promoted apoptosis in a wide range of human cancers (9–12). However, little is known concerning the antitumor activity of Sch B on cholangiocarcinoma (CCA) cells and its underlying mechanisms. In the present study, for the first time, we examined the inhibitory effect and mechanism of Sch B on CCA cells. We showed that Sch B dose-dependently decreased cell viability and induced cell cycle arrest and apoptosis in CCA cells. Our in vivo study showed that Sch B strongly suppressed tumor growth. Thus, Sch B may be a promising drug for CCA prevention and treatment.

To examine the mechanism of Sch B-induced inhibition of cell survival, we performed the cell cycle distribution experiment in the presence of Sch B and found that it induced G0/G1 phase arrest. Further study showed that Sch B treatment resulted in a downregulation of the expression of cyclin D1 and CDK4 in both HCCC-9810 and RBE cells (Fig. 3C). It is well known that the cell cycle is a tightly regulated process consisting of 4 distinct phases: G0/G1, S, G2 and M. Activation of each phase is dependent on the regulation of various cyclins and cyclin-dependent kinases (Cdks) (16,17). The complex of cyclin D1 and CDK4 is the main driver of the transition of cells from G0/G1 to S phase by phosphorylating of retinoblastoma (Rb) (18–20). Hyper-phosphorylated Rb activates E2F after its dissociation from the E2F/DP1/Rb complex (21). As suggested by our cell cycle analysis data, Sch B arrested HCCC-9810 and RBE cells at the G0/G1 phase (Fig. 3A), which may be due to the downregulation of cyclin D1 and CDK4.

Apoptosis, genetically programmed cell death that plays crucial roles in cell death and survival, is considered to be one of the main contributors to cancer development. Chemical compounds that induce cancer cell apoptosis are considered promising anticancer drugs (22,23). Caspases, a family of cysteine proteases, play essential roles in apoptosis. Both the death-receptor-induced extrinsic pathway and the mitochondria-apoptosome-mediated intrinsic pathway ultimately activate caspases (24,25). Among them, caspase-3, which is activated by caspase-8 or -9, is one of the most important executioner caspases (26). Caspase-3 cleaves several cellular proteins, including the PARP protein, resulting in morphological changes and DNA fragmentation that eventually lead to apoptosis (27). In the present study, we observed the activation of caspase-9 and -3 and the cleavage of PARP following Sch B treatment in HCCC-9810 and RBE cells, indicating that the mitochondrial pathway was involved in Sch B-induced apoptosis.

Bcl-2 family proteins, including Bax, Bad, Bid, Bcl-2 and Bcl-xL, play essential roles in the mitochondria-mediated apoptosis pathway by regulating the release of cytochrome c (28). The pro-apoptotic members Bax and Bad induce the release of cytochrome c from the mitochondria within cells, whereas anti-apoptotic Bcl-2 and Bcl-xL promote cell survival by preventing cytochrome c release from the mitochondria (29,30). A low Bcl-2 to Bax ratio can induce ΔΨm collapse, the release of cytochrome c, and subsequent apoptosis (31). The present study showed that the apoptosis that occurs in response to Sch B treatment is accompanied by decreased expression of anti-apoptotic genes and increased expression of pro-apoptotic genes. Consistent with this result, an obvious decrease of ΔΨm was observed in CCA cells treated with Sch B. Taken together, these results indicate that the mitochondrial pathway is involved in Sch B-induced apoptosis. Sch B may be a promising drug for CCA treatment. However, further studies are certainly needed to elucidate the mechanism underlying Sch B-induced apoptosis.

Acknowledgments

The present study was supported by grants from the Major Science and Technology Projects of Zhejiang Province (2014C04008-1).

References

  • 1.de Groen PC, Gores GJ, LaRusso NF, Gunderson LL, Nagorney DM. Biliary tract cancers. N Engl J Med. 1999;341:1368–1378. doi: 10.1056/NEJM199910283411807. [DOI] [PubMed] [Google Scholar]
  • 2.Tyson GL, Ilyas JA, Duan Z, Green LK, Younes M, El-Serag HB, Davila JA. Secular trends in the incidence of cholangiocarcinoma in the USA and the impact of misclassification. Dig Dis Sci. 2014;59:3103–3110. doi: 10.1007/s10620-014-3276-2. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 3.Landis SH, Murray T, Bolden S, Wingo PA. Cancer statistics, 1998. CA Cancer J Clin. 1998;48:6–29. doi: 10.3322/canjclin.48.1.6. [DOI] [PubMed] [Google Scholar]
  • 4.Patel T. Worldwide trends in mortality from biliary tract malignancies. BMC Cancer. 2002;2:10. doi: 10.1186/1471-2407-2-10. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 5.Khan SA, Davidson BR, Goldin R, Pereira SP, Rosenberg WM, Taylor-Robinson SD, Thillainayagam AV, Thomas HC, Thursz MR, Wasan H. British Society of Gastroenterology: Guidelines for the diagnosis and treatment of cholangiocarcinoma: Consensus document. Gut. 2002;51(Suppl 6):VI1–VI9. doi: 10.1136/gut.51.suppl_6.vi1. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 6.Zhang TC, Cao EH, Li JF, Ma W, Qin JF. Induction of apoptosis and inhibition of human gastric cancer MGC-803 cell growth by arsenic trioxide. Eur J Cancer. 1999;35:1258–1263. doi: 10.1016/S0959-8049(99)00106-9. [DOI] [PubMed] [Google Scholar]
  • 7.Shaib Y, El-Serag HB. The epidemiology of cholangiocarcinoma. Semin Liver Dis. 2004;24:115–125. doi: 10.1055/s-2004-828889. [DOI] [PubMed] [Google Scholar]
  • 8.Liu GT. Pharmacological actions and clinical use of fructus schizandrae. Chin Med J. 1989;102:740–749. [PubMed] [Google Scholar]
  • 9.Li L, Wang T, Xu ZL, Yu Y, Chen W, Chen F. Effects of schisandrin B on reversing multidrug resistance in human breast cancer cells transfected with mdr1 gene. Zhonghua Yi Xue Za Zhi. 2005;85:1633–1637. In Chinese. [PubMed] [Google Scholar]
  • 10.Liu XN, Zhang CY, Jin XD, Li YZ, Zheng XZ, Li L. Inhibitory effect of schisandrin B on gastric cancer cells in vitro. World J Gastroenterol. 2007;13:6506–6511. doi: 10.3748/wjg.13.6506. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 11.Wu YF, Cao MF, Gao YP, Chen F, Wang T, Zumbika EP, Qian KX. Down-modulation of heat shock protein 70 and up-modulation of caspase-3 during schisandrin B-induced apoptosis in human hepatoma SMMC-7721 cells. World J Gastroenterol. 2004;10:2944–2948. doi: 10.3748/wjg.v10.i20.2944. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 12.Li Q, Lu XH, Wang CD, Cai L, Lu JL, Wu JS, Zhuge QC, Zheng WM, Su ZP. Antiproliferative and apoptosis-inducing activity of schisandrin B against human glioma cells. Cancer Cell Int. 2015;15:12. doi: 10.1186/s12935-015-0160-x. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 13.Liu Z, Zhang B, Liu K, Ding Z, Hu X. Schisandrin B attenuates cancer invasion and metastasis via inhibiting epithelial-mesenchymal transition. PLoS One. 2012;7:e40480. doi: 10.1371/journal.pone.0040480. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 14.Nishida H, Tatewaki N, Nakajima Y, Magara T, Ko KM, Hamamori Y, Konishi T. Inhibition of ATR protein kinase activity by schisandrin B in DNA damage response. Nucleic Acids Res. 2009;37:5678–5689. doi: 10.1093/nar/gkp593. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 15.Hu YP, Tan ZJ, Wu XS, Liu TY, Jiang L, Bao RF, Shu YJ, Li ML, Weng H, Ding Q, et al. Triptolide induces s phase arrest and apoptosis in gallbladder cancer cells. Molecules. 2014;19:2612–2628. doi: 10.3390/molecules19022612. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 16.Bloom J, Cross FR. Multiple levels of cyclin specificity in cell-cycle control. Nat Rev Mol Cell Biol. 2007;8:149–160. doi: 10.1038/nrm2105. [DOI] [PubMed] [Google Scholar]
  • 17.Nigg EA. Cyclin-dependent protein kinases: Key regulators of the eukaryotic cell cycle. BioEssays. 1995;17:471–480. doi: 10.1002/bies.950170603. [DOI] [PubMed] [Google Scholar]
  • 18.Harbour JW, Luo RX, Dei Santi A, Postigo AA, Dean DC. Cdk phosphorylation triggers sequential intramolecular interactions that progressively block Rb functions as cells move through G1. Cell. 1999;98:859–869. doi: 10.1016/S0092-8674(00)81519-6. [DOI] [PubMed] [Google Scholar]
  • 19.Ezhevsky SA, Ho A, Becker-Hapak M, Davis PK, Dowdy SF. Differential regulation of retinoblastoma tumor suppressor protein by G1 cyclin-dependent kinase complexes in vivo. Mol Cell Biol. 2001;21:4773–4784. doi: 10.1128/MCB.21.14.4773-4784.2001. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 20.Hinds PW, Mittnacht S, Dulic V, Arnold A, Reed SI, Weinberg RA. Regulation of retinoblastoma protein functions by ectopic expression of human cyclins. Cell. 1992;70:993–1006. doi: 10.1016/0092-8674(92)90249-C. [DOI] [PubMed] [Google Scholar]
  • 21.Massagué J. G1 cell-cycle control and cancer. Nature. 2004;432:298–306. doi: 10.1038/nature03094. [DOI] [PubMed] [Google Scholar]
  • 22.Chinkwo KA. Sutherlandia frutescens extracts can induce apoptosis in cultured carcinoma cells. J Ethnopharmacol. 2005;98:163–170. doi: 10.1016/j.jep.2005.01.016. [DOI] [PubMed] [Google Scholar]
  • 23.Asgar MA, Senawong G, Sripa B, Senawong T. Synergistic anticancer effects of cisplatin and histone deacetylase inhibitors (SAHA and TSA) on cholangiocarcinoma cell lines. Int J Oncol. 2016;48:409–420. doi: 10.3892/ijo.2015.3240. [DOI] [PubMed] [Google Scholar]
  • 24.Hu W, Kavanagh JJ. Anticancer therapy targeting the apoptotic pathway. Lancet Oncol. 2003;4:721–729. doi: 10.1016/S1470-2045(03)01277-4. [DOI] [PubMed] [Google Scholar]
  • 25.Reed JC. Apoptosis-regulating proteins as targets for drug discovery. Trends Mol Med. 2001;7:314–319. doi: 10.1016/S1471-4914(01)02026-3. [DOI] [PubMed] [Google Scholar]
  • 26.Zheng L, Zheng J, Wu LJ, Zhao YY. Julibroside J8-induced HeLa cell apoptosis through caspase pathway. J Asian Nat Prod Res. 2006;8:457–465. doi: 10.1080/10286020500173309. [DOI] [PubMed] [Google Scholar]
  • 27.Antonsson B. Mitochondria and the Bcl-2 family proteins in apoptosis signaling pathways. Mol Cell Biochem. 2004;256–257:141–155. doi: 10.1023/B:MCBI.0000009865.70898.36. [DOI] [PubMed] [Google Scholar]
  • 28.Pal S, Pal PB, Das J, Sil PC. Involvement of both intrinsic and extrinsic pathways in hepatoprotection of arjunolic acid against cadmium induced acute damage in vitro. Toxicology. 2011;283:129–139. doi: 10.1016/j.tox.2011.03.006. [DOI] [PubMed] [Google Scholar]
  • 29.Tsujimoto Y. Bcl-2 family of proteins: Life-or-death switch in mitochondria. Biosci Rep. 2002;22:47–58. doi: 10.1023/A:1016061006256. [DOI] [PubMed] [Google Scholar]
  • 30.Das A, Banik NL, Patel SJ, Ray SK. Dexamethasone protected human glioblastoma U87MG cells from temozolomide induced apoptosis by maintaining Bax:Bcl-2 ratio and preventing proteolytic activities. Mol Cancer. 2004;3:36. doi: 10.1186/1476-4598-3-36. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 31.Zhang YH, Wu YL, Tashiro S, Onodera S, Ikejima T. Reactive oxygen species contribute to oridonin-induced apoptosis and autophagy in human cervical carcinoma HeLa cells. Acta Pharmacol Sin. 2011;32:1266–1275. doi: 10.1038/aps.2011.92. [DOI] [PMC free article] [PubMed] [Google Scholar]

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