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Introduction

Cisplatin (cis-diamminedichloroplatinum II) is one of the clinical chemotherapeutic agents used against a broad spectrum of human malignancies, such as ovarian, cervical, prostate and lung cancer (1). However, relapse following cisplatin therapy is inevitable. Thus, it is particularly important to elucidate the cell-killing mechanism of cisplatin (2–4). Cisplatin is generally considered to kill cancer cells by damaging DNA and inhibiting DNA synthesis, which induces mitochondria-mediated apoptosis and consequently, cell death (5–8). Recent findings have revealed that cisplatin triggers apoptotic events via endoplasmic reticulum (ER) stress (9,10).

The ER is a crucial organelle in eukaryotic cells that is essential for the biological processes required for cell survival and normal cell function, such as protein folding and secretion, lipid biosynthesis and calcium homeostasis. Multiple stimuli can cause the accumulation of unfolded and incompletely folded proteins in the ER, which initiates the unfolded protein response (UPR) and ER stress (11,12). In the resting state, the ER, an intracellular store of calcium, regulates basic calcium oscillations via calcium ion channels on the ER membrane in order to transmit intracellular biological information. Once balance is disrupted, a regulatory network of downstream signaling pathways is activated (13–15). Previous studies have suggested that chemotherapeutic agents target the metabolism of reactive oxygen species and ATP production in the mitochondria, activate mitochondria-mediated cell apoptosis, and inhibit cell growth and proliferation via an increase in cellular calcium mobilization (16–18). However, the function of calcium signaling in ER-derived apoptosis induced by chemotherapy drugs is not clear.

Thus, we presume that calcium signaling plays an important role in the mitochondria-mediated and ER-mediated apoptosis pathways following cisplatin exposure in human cervical cancer HeLa cells. In the present study, it was found that treatment with cisplatin significantly increased cellular calcium concentrations and triggered the mitochondria-dependent and ER-dependent apoptosis pathways in HeLa cells, which could be inhibited by blocking calcium signaling. These results demonstrated that calcium efflux from the ER plays a significant role in the regulation of apoptosis triggered by cisplatin in HeLa cells.

Materials and methods

Reagents and antibodies

In the present study, the cisplatin, bis-(o-aminophenoxy)ethane-N,N,N',N'-tetra-acetic acid acetoxymethyl ester (BAPTA/AM), inositol triphosphate receptor (IP3R) inhibitor 2-aminoethyl diphenylborinate (2-APB) and 3-(4,5-dimetrylthiazol-2-yl)-2,5-diphenyltetrazolium bromide (MTT) were purchased from Sigma-Aldrich (St. Louis, MO, USA). Fetal bovine serum (FBS) and Iscove's modified Dulbecco's medium (IMDM) were purchased from Life Technologies (Thermo Fisher Scientific Inc., Waltham, MA, USA). Fluo-4/AM, Alexa Fluor 546 donkey polyclonal anti-rabbit immunoglobulin (Ig)G (catalog no., A10040), Alexa Fluor 546 donkey polyclonal anti-mouse IgG (catalog no., A10036) and Alexa Fluor 488 donkey polyclonal anti-rabbit IgG (catalog no., A-21206) were purchased from Invitrogen (Thermo Fisher Scientific Inc.). Rhod-2/AM was purchased from AAT Bioquest Inc. (Sunnyvale, CA, USA). Enhanced chemiluminescence (ECL) reagents were obtained from Thermo Fisher Scientific Inc. Mouse monoclonal anti-C/EBP homologous protein (CHOP; catalog no., ab11419), rabbit polyclonal anti-caspase-3 (catalog no., ab13847) and rabbit polyclonal anti-activated-caspase-3 (catalog no., ab2302) antibodies were purchased from Abcam (Cambridge, MA, USA), while rabbit polyclonal anti-caspase-4 (catalog no., 24287) and rabbit polyclonal anti-calpain-1 catalytic subunit (CAPN1; catalog no., 32201) antibodies were purchased from Signalway Antibody Co. (College Park, MD, USA), and mouse monoclonal anti-glucose-regulated protein (GRP78; 78 kDa; catalog no., sc-376768) antibody was purchased from Santa Cruz Biotechnology Inc. (Dallas, TX, USA). Rabbit polyclonal anti-β-actin (catalog no., 20536-1-AP) and peroxidase-conjugated Affinipure goat anti-mouse- and anti-rabbit Ig were purchased from Proteintech Group Inc. (Chicago, IL, USA; catalog nos., SA00001-1 and SA00001-2). All other reagents and antibodies were purchased from Changchun Baoxin Biotechnology Co. (Changchun, China).

Cell culture

Human cervical cancer HeLa cells were obtained from China Academy of Chinese Medical Sciences (Beijing, China), and were cultured at 37°C in a 5% (v/v) CO2 and 95% (v/v) air atmosphere, using IMDM containing 10% (v/v) FBS, and 100 U/ml penicillin and 100 µg/ml streptomycin. The cells were divided into six groups: Non-treated cells, cells treated with 5 µg/ml cisplatin, cells treated with 2.5 µM BAPTA/AM, cells treated with 100 µM 2-APB, cells treated with 5 µg/ml cisplatin combined with 2.5 µM BAPTA/AM, and cells treated with 5 µg/ml cisplatin combined with 100 µM 2-APB.

Determination of intracellular and mitochondrial free Ca2+ levels

The fluorescent calcium indicator Fluo-4/AM (5 µM) and Rhod-2 (5 µM) were used to measure intracellular and mitochondrial free Ca2+ levels, as previously described (19). The cells were monitored using an Olympus FV1000 confocal laser microscope (Olympus Corporation, Tokyo, Japan). Fluorescence images labeled with Fluo-4/Rhod-2 were collected using an excitation wavelength of 488/546 nm. The same parameters of illumination and detection were maintained digitally for consistency throughout the experiments.

MTT assay

Cell viability was determined using the MTT assay. In the experiments, exponentially growing HeLa cells were seeded in 96-well culture plates at a density of 1×104 cells/well. After 24 h of incubation, cisplatin with or without BAPTA/AM and 2-APB was added for 24 h in four parallel wells. MTT solution (5 mg/ml) was added for 4 h, followed by the addition of 150 µl dimethyl sulfoxide. After 10 min of shaking, the absorbance was measured at 570 nm using a microplate reader (iMark; Bio-Rad Laboratories, Inc., Hercules, CA, USA). The survival rate was calculated as follows: Survival (%) = absorbance of experimental group / absorbance of control group × 100. In each experiment, the mean value of four wells per treatment group was calculated.

Flow cytometry analysis

The MUSE™ Annexin-V Dead Cell kit (EMD Millipore, Billerica, MA, USA) was used to monitor cell death. In the experiments, exponentially growing HeLa cells were seeded in 6-well culture plates at a density of 2×105 cells/well. Following exposure to the different experimental conditions, the cells were trypsinized and resuspended in IMDM medium with 10% FBS at a concentration of 1×106 cells/ml. The cells were incubated with Annexin-V in the dark at room temperature for 20 min. Finally, samples were detected using the MUSE Cell Analyzer (EMD Millipore). All experiments were performed in triplicate.

Immunofluorescence staining and confocal laser microscopy

The cells were cultured on coverslips overnight, and after treatment with the indicated dose of cisplatin with or without BAPTA/AM and 2-APB for 24 h, were fixed with 4% (w/v) paraformaldehyde, stained with nuclear Hoechst 33342 (1 µg/ml; Sigma-Aldrich) for 5 min, washed with phosphate-buffered solution (PBS), and examined using an Olympus FV1000 confocal laser microscope to reveal cell chromatin condensation. The expression of GRP78, active caspase-3 and CHOP was examined by indirect immunofluorescence. The cells were cultured on coverslips overnight, then treated with the indicated dose of cisplatin with or without BAPTA/AM and 2APB for 24 h, and rinsed with PBS three times. After incubation, the cells were fixed with 4% (w/v) paraformaldehyde for 20 min, permeabilized with 0.1% (v/v) Triton X-100 for 5 min, blocked with bovine serum albumin, and incubated with the primary antibodies for GRP78 (1:50 dilution), active caspase-3 (1:250 dilution), and CHOP (1:100 dilution) overnight at 4°C. The cells were then incubated in Alexa Fluor 488 Donkey Anti-Rabbit IgG, Alexa Fluor 546 Donkey Anti-Rabbit IgG and Alexa Fluor 546 Donkey Anti-Mouse IgG secondary antibodies (1:400 dilution) for 30 min, stained with Hoechst 33342 (1 µg/ml) for 5 min and washed with PBS three times. After mounting, the cells were examined under an Olympus FV1000 confocal laser microscope. The same parameters of illumination and detection were maintained digitally throughout the experiments.

Western blotting

Whole-cell protein extracts from the HeLa cells were prepared with cell lysis buffer [50 mM Tris-HCl (pH 7.5), 150 mM NaCl, 1 mM sodium-EDTA, 1 mM EDTA, 1% (v/v) Triton X-100, 2.5 mM sodium pyrophosphate, 1 mM β-glycerophosphate, 1 mM Na3VO4, 1 mM NaF, 1 µg/ml leupeptin and 1 mM PMSF] for western blotting. Protein concentration was quantified using the BCA Protein Assay kit (Pierce™; Thermo Fisher Scientific Inc.). For western blot analysis, lysates (30 µg) were resolved on 10% (w/v) sodium dodecyl sulfate-polyacrylamide gels and transferred onto immobilon-P transfer membranes (EMD Millipore). The membranes were blocked with 5% (w/v) skimmed dry milk in buffer [10 mM Tris-HCl (pH 7.6), 100 mM NaCl and 0.1% Tween 20] for 1 h at room temperature and then incubated with the desired primary antibody overnight at 4°C, followed by incubation with horseradish peroxidase-conjugated secondary antibody (1:2,000; Proteintech Group Inc.) for 1.5 h at room temperature. Immunodetection was performed using the ECL reagents and images were captured using Syngene Bio Imaging (Synoptics, Cambridge, UK). The level of protein was normalized to that of actin and the ratios of normalized protein to actin are presented as the mean ± standard deviation from three independent experiments. Protein levels were quantified by densitometry using Quantity One version 4.6.2 software (Bio-Rad Laboratories Inc.).

Statistical analysis

Data are representative of three independent experiments each performed in triplicate. Statistical analysis of the data was performed using a one-way analysis of variance on IBM SPSS version 22.0 (IBM SPSS, Armonk, NY, USA). Tukey's post-hoc test was used to determine the significance for all pairwise comparisons of interest. P<0.05 was considered to indicate a statistically significant difference.

Results

Cisplatin increases free Ca2+ levels in the cytosol and mitochondria

For the determination of cytosolic and mitochondrial free Ca2+ levels, the Ca2+-sensitive fluorescent dyes, Fluo-4/AM and Rhod-2/AM, were used. Based on previous studies (10), the HeLa cells were treated with increasing doses of cisplatin (2.5, 5 and 10 µg/ml) for 0, 6, 12 and 24 h, and further incubated with the calcium indicators Fluo-4/AM and Rhod-2/AM. Confocal microscopy was used to observe alterations in free Ca2+ levels. It was found that the free Ca2+ levels in the cytosol (Fig. 1A and B) and mitochondria (Fig. 1C and D) increased in a dose- and time-dependent manner in the HeLa cells (P<0.001).

Figure 1. Cisplatin increases free Ca2+ levels in the cytosol and mitochondria. (A) The cells were treated with cisplatin (2.5, 5 or 10 µg/ml) for 0, 6, 12 and 24 h, and incubated with the fluorescent calcium indicator, Fluo-4/AM. Calcium concentrations in the cytosol were observed by confocal microscopy (scale bar, 40 µm). (B) Quantitation of free Ca2+ levels in the cytosol. Data are presented as the mean ± SD (n=3). *P<0.05 vs. control. (C) Cells were treated with cisplatin (2.5, 5 or 10 µg/ml) for 0, 6, 12 and 24 h, and incubated with the fluorescent calcium indicator, Rhod-2. Calcium concentrations in the mitochondria were observed by confocal microscopy (scale bar, 40 µm). (D) Quantitation of free Ca2+ levels in the mitochondria. Data are presented as the mean ± SD (n=3). *P<0.05 vs. control. SD, standard deviation.

These results suggested that cisplatin increases free Ca2+ levels in the cytosol and mitochondria of HeLa cells, indicating the relevance of calcium in the cell death induced by cisplatin.

Calcium signaling is involved in cisplatin-induced mitochondria-dependent apoptosis

To evaluate the action of calcium in cisplatin-induced apoptotic cell death, the calcium chelating agent, BAPTA/AM, and the IP3R inhibitor, 2-APB, were used to alter the free Ca2+ levels induced by cisplatin. It was observed that the cisplatin-induced free Ca2+ levels in the cytosol and mitochondria substantially decreased in the groups treated with cisplatin combined with BAPTA/AM or 2-APB (Fig. 2A and B).

Figure 2. Inhibition of calcium signaling decreases the level of free Ca2+ in the cytosol and mitochondria, and inhibits cell growth. (A) HeLa cells were treated with cisplatin (5 µg/ml) with or without BAPTA/AM (2.5 µM) and 2-APB (100 µM) for 12 and 24 h. The cells were incubated with the fluorescent calcium indicator, Fluo-4/AM. Calcium concentrations in the cytosol were observed by confocal microscopy (scale bar, 40 µm). (B) HeLa cells were treated with cisplatin (5 µg/ml) with or without BAPTA/AM (2.5 µM) and 2-APB (100 µM) for 12 and 24 h, and incubated with the fluorescent calcium indicator, Rhod-2. Calcium concentrations in the mitochondria were observed by confocal microscopy (scale bar, 30 µm). (C) HeLa cells were treated with cisplatin (5 µg/ml) with or without BAPTA/AM (2.5 µM) and 2-APB (100 µM) for 24 h. Cell viability was determined using the 3-(4,5-dimetrylthiazol-2-yl)-2,5-diphenyltetrazolium bromide assay. Data are presented as the mean ± standard deviation (n=3). *P<0.05 vs. control; #P<0.05 vs. cisplatin. (D) HeLa cells were treated with cisplatin (5 µg/ml) with or without BAPTA/AM (2.5 µM) and 2-APB (100 µM) for 24 h. Cell morphology was observed using an inverted phase contrast microscope at x100 magnification. BAPTA/AM, bis-(o-aminophenoxy)ethane-N,N,N',N'-tetra-acetic acid acetoxymethyl ester; 2-APB, 2-aminoethyl diphenylborinate.

The MTT assay was used to detect cell viability. The results demonstrated that cisplatin inhibited cell viability in the HeLa cells. Treatment combined with BAPTA/AM or 2-APB decreased the cytotoxic effects of cisplatin (P<0.001), while treatment with BAPTA/AM or 2-APB alone had no significant effect on cell viability (Fig. 2C). At the same time, an optical microscope was used to examine cellular morphological changes. Compared with the controls, the cells treated with cisplatin became round and fragmented. The numbers of rounded and fragmented cells in the cultures treated with cisplatin combined with BAPTA/AM or 2-APB were less than that in the group treated with only cisplatin (Fig. 2D).

Based on the MTT results, flow cytometry was used to detect the ratio of cell apoptosis induced by cisplatin in the HeLa cells. Consistent with the MTT results, the rate of apoptosis in the cells treated with cisplatin combined with BAPTA/AM or 2-APB (37.8 and 36.1%, respectively) was lower than that of the cells treated only with cisplatin (55.3%) (Fig. 3A). Using confocal microscopy, apoptotic chromatin condensation was examined with Hoechst 33342 staining. Treatment with cisplatin alone induced significant apoptotic chromatin condensation in the HeLa cells, while the cells treated with cisplatin combined with BAPTA/AM or 2-APB showed a lower ratio of apoptotic chromatin condensation (Fig. 3B).

Figure 3. Inhibition of calcium signaling decreases cisplatin-induced mitochondria-mediated apoptosis in HeLa cells. (A) HeLa cells were treated with cisplatin (5 µg/ml) with or without BAPTA/AM (2.5 µM) and 2-APB (100 µM) for 24 h and then stained with Annexin-V. Data are presented as the mean ± SD (n=3). (B) HeLa cells were treated with cisplatin (5 µg/ml) with or without BAPTA/AM (2.5 µM) and 2-APB (100 µM) for 24 h, and stained with Hoechst 33342. Cell morphology was observed by confocal microscopy (scale bar, 30 µm). (C) The expression of calpain, caspase-3 and cleaved caspase-3 in HeLa cells treated with cisplatin (5 µg/ml) with or without BAPTA/AM (2.5 µM) and 2-APB (100 µM) for 12 h by western blotting. (D) Quantitation of calpain and cleaved caspase-3 protein levels. Data are presented as the mean ± SD (n=3). *P<0.05 vs. control; #P<0.05 vs. cisplatin. (E) The expression of cleaved caspase-3 was detected by confocal microscopy following the various treatments for 12 h (scale bar, 20 µm). BAPTA/AM, bis-(o-aminophenoxy)ethane-N,N,N',N'-tetra-acetic acid acetoxymethyl ester; 2-APB, 2-aminoethyl diphenylborinate; SD, standard deviation.

CAPN1 (also known as µ-calpain) is a Ca2+-dependent cysteine protease, and its activation requires high levels of free calcium in the cytosol (20,21). Thus, the present study assessed calcium levels and apoptosis in the HeLa cells by monitoring the expression of CAPN1 and cleaved caspase-3 by western blotting. As shown in Fig. 3C and D, cisplatin enhanced the expression of CAPN1 and cleaved caspase-3 (P<0.001). Meanwhile, treatment with cisplatin combined with BAPTA/AM or 2-APB decreased the level of CAPN1 and cleaved caspase-3 induced by cisplatin. Consistent with the western blotting results, immunofluorescence against caspase-3 revealed a similar effect (Fig. 3E). These results indicated that cisplatin upregulates intracellular calcium mobilization and initiates apoptotic events.

Cisplatin-induced pro-apoptosis calcium signaling is derived from ER stress

Cisplatin has been reported to induce ER stress and downstream processes associated with apoptosis (7,10,22). To further verify if the resultant apoptosis was partially induced by ER stress, the present study assessed the occurrence of ER stress and ER-associated apoptosis by examining the expression levels of ER stress-associated proteins.

The expression of GRP78, an ER molecular chaperone that induces ER stress upon accumulation, was detected. Western blotting revealed that cisplatin upregulated the expression of GRP78, and that combined treatment with BAPTA/AM or 2-APB downregulated the expression of GRP78 (Fig. 4A and B; P<0.001). Using confocal microscopy, it was observed that the accumulation of GRP78 increased in cells treated with cisplatin only, while combined treatment with BAPTA/AM or 2-APB markedly decreased the cisplatin-induced GRP78 accumulation (Fig. 4C).

Figure 4. Inhibition of calcium signaling decreases cisplatin-induced ER stress-mediated apoptosis in HeLa cells. (A) Western blotting detection of ER stress proteins in HeLa cells treated with cisplatin (5 µg/ml) with or without BAPTA/AM (2.5 µM) and 2-APB (100 µM) for 12 h. (B) Quantitation of ER stress protein levels. Data are presented as the mean ± standard deviation (n=3). *P<0.05 vs. control; #P<0.05 vs. cisplatin. (C) The expression of GRP78 was detected by confocal microscopy following various treatments for 12 h (scale bar, 20 µm). (D) The expression of CHOP was detected by confocal microscopy following various treatments for 12 h (scale bar, 20 µm). BAPTA/AM, bis-(o-aminophenoxy)ethane-N,N,N',N'-tetra-acetic acid acetoxymethyl ester; 2-APB, 2-aminoethyl diphenylborinate; CHOP, C/EBP homologous protein; GRP78, glucose-regulated protein, 78 kDa; ER, endoplasmic reticulum.

Next, the ER stress-associated apoptotic proteins, caspase-4 and CHOP, were monitored. Western blotting revealed that cisplatin enhanced the expression of CHOP and cleaved caspase-4, while combined treatment with BAPTA/AM or 2-APB inhibited these effects (Fig. 4A and B; P<0.001). Similarly, confocal microscopy revealed marked accumulation of CHOP in cells treated with cisplatin alone, and low-level CHOP accumulation in groups treated with cisplatin combined with BAPTA/AM or 2-APB (Fig. 4D).

These results demonstrated that cisplatin induced pro-apoptotic calcium signaling, which resulted in ER stress-mediated apoptotic events in the HeLa cells.

Discussion

Cisplatin is one of several effective antitumor drugs widely used against multiple solid tumors in the clinic; it acts by damaging DNA, inhibiting DNA synthesis and inducing apoptosis in cancer cells (5,23). Previous studies have reported that chemotherapy drugs, including cisplatin, cause mitochondrial dysfunction, the release of cytochrome c, the activation of the caspase-mediated cascade and apoptotic cell death (24–27). In the present study, it was found that cisplatin inhibited cell growth, upregulated active caspase-3 and induced the mitochondria-mediated apoptosis pathway in human HeLa cells (Figs. 2 and 3). An increasing amount of evidence has indicated that cisplatin induces cell apoptosis through ER stress (9,10,22). The ER is an important organelle in eukaryotic cells, and is involved in several critical processes. Under stressful conditions, numerous unfolded and incompletely folded proteins accumulate in the ER lumen, which stimulates the UPR, leading to ER stress (11,12). It is generally considered that the accumulation of the calcium-dependent molecular chaperone, GRP78, initiates ER stress (10,28). The results of the present study indicated that treatment with cisplatin induces the accumulation of GRP78 in HeLa cells and results in ER stress (Fig. 4A and C). The transcription factor CHOP (also known as DNA damage-inducible transcript 3) is an ER stress-associated apoptosis protein that integrates the apoptotic endoplasmic reticulum to nucleus signaling 1, eukaryotic translation initiation factor 2α kinase 3 and activating transcription factor 6 pathways in the UPR (29–32). Caspase-4 is a calcium-dependent caspase; its overexpression stimulates the downstream cascade reaction and leads to cell apoptosis, which is caused by destruction of the ER and calcium pool emptying (33–35). Thus, the present study examined the expression of these two ER stress-associated apoptotic proteins. The results demonstrated that cisplatin markedly increased the expression levels of these two proteins (Fig. 4A and B). These data suggested that in addition to the mitochondria-mediated apoptotic pathway, cisplatin could also induce cell apoptosis via ER stress. Notably, concurrently with the occurrence of apoptosis, the cytosolic and mitochondrial free Ca2+ levels increased, and calpain expression was upregulated. The modulation of calcium concentration in the cytoplasm affected the activation of the calpains, which are evolutionarily conserved Ca2+-dependent cysteine proteases (36,37). It is reported that the overexpression of calpains promotes the cleavage of Bid, which in turn modulates Bax and activates caspase-3. There is also evidence to suggest that activation of caspase-4 requires calpains (38–40). The aforementioned results suggest that calcium signaling involves two apoptotic pathways: i) Calcium ion entry into the mitochondria, which induces calcium disorder in he mitochondria and leads to mitochondria-mediated apoptosis; and ii) calcium signaling in the cytosol activates calcium-dependent proteases and results in the expression of ER stress-associated apoptotic proteins.

To investigate this hypothesis, the calcium chelating agent, BAPTA/AM, was used to block free Ca2+ in the cytoplasm. Won et al reported that apoptosis induced by 3α,23-isopropylidenedioxyolean-12-en-27-oic acid was substantially reduced following combined treatment with BAPTA/AM in HeLa cells (40). In the present study, HeLa cells were treated with cisplatin combined with BAPTA/AM. The data demonstrated that calcium concentrations in the cytoplasm and expression levels of calpain were reduced in the presence of BAPTA/AM. Moreover, in the group treated with cisplatin combined with BAPTA/AM, the ER-stress proteins CHOP and active caspase-4 were downregulated (Fig. 4A and B). These results indicated that endogenous calcium efflux participates in ER stress-mediated apoptosis induced by cisplatin in HeLa cells. Intercellular calcium homeostasis is controlled by calcium ion channels on the ER membrane, which include IP3R, ryanodine receptors and sarcoendoplasmic reticular Ca2+-ATPase pumps (41,42). To further confirm the source of calcium signaling, the IP3R inhibitor, 2-APB, was used to inhibit calcium release from the ER. Yoon et al reported that 2-APB potently inhibited calcium release from the ER and suppressed celastrol-induced apoptosis in breast cancer cell lines (MDA-MB 435S and MCF-7) (43). In the present study, it was found that combined treatment with 2-APB decreased calcium release from the ER and inhibited cisplatin-induced apoptosis in the HeLa cells. The data revealed that these inhibitory effects mainly manifested via two mechanisms: i) 2-APB inhibits calcium flux from the ER to the mitochondria and decreases the expression of cleaved caspase-3, which attenuates mitochondria-mediated apoptosis; and ii) 2-APB blocks calcium flux from the ER to the cytosol, inhibits the activation of calpains, and downregulates the expression of the ER stress proteins, CHOP and caspase-4. These results suggested that blocking calcium release from the ER effectively mitigates the ER stress-associated apoptotic pathway. Previous studies have revealed that cisplatin initiates ER stress and interferes with calcium homeostasis (44,45). The present study found that blocking calcium efflux decreased the level of ER stress correspondingly. This phenomenon suggests that calcium signaling may act as a positive feedback mechanism by modulating ER stress. However, further investigations are required.

In summary, the present study demonstrated that cisplatin induced ER stress and led to apoptosis in human HeLa cells. Notably, treatment with cisplatin combined with BAPTA/AM or 2-APB markedly decreased the inhibition of cell growth and the rate of apoptosis. The results demonstrate that calcium efflux from the ER regulates cell apoptosis triggered by cisplatin in HeLa cells. In addition, the study provided further mechanistic insights into the tumor cell-killing effect of cisplatin and potential therapeutic strategies to improve cisplatin chemotherapy.

Acknowledgements

This research was supported by the National Natural Science Foundation of China (grant nos. 81272876 and 81372793) and the Department of Education of Jilin Province Project (grant no. 2013361).

References