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Introduction

Histone acetylation is an important step in the initiation of transcription (1). The acetylation of lysine residues in histones weakens their binding to DNA and leads to euchromatin structure, which induces transcriptional factors to bind to promoter regions of genes (2). Two opposing enzyme activities of histone acetyltransferases (HATs) and histone deacetylases (HDACs) determine the acetylation status of histones, respectively, acetylating or deacetylating the epsilon-amino groups of lysine residues located in the amino-terminal tails of the histones (2). It was reported that dysregulation of HDAC activity can cause the silence of tumor suppressor genes such as p53 and contribute to cancer initiation (3,4). Previous studies have demonstrated that HDAC activity and expression are increased in many human cancers including prostate and pancreatic cancer (5,6). Therefore, HDAC inhibitors have been considered as novel anticancer drugs. In particular, the reversible HDAC inhibitor, trichostatin A (TSA) and its hydroxamate analogues can effectively and selectively induce tumor growth arrest at very low concentrations (nano- to micromolar range) (7). In fact, vorinostat (suberoylanilide hydroxamic acid) has been used for the treatment of cutaneous T-cell lymphoma (8). Other types of HDAC inhibitors such as romidepsin, panobinostat and valproic acid are clinically evaluated in cancer therapy (9,10). In general, HDAC inhibitors can induce cell cycle arrest, cell death and cell differentiation in various cancer cells (11–13). They have also been shown to generate reactive oxygen species (ROS) in solid tumor and leukemia cells (14). Excessive production of ROS, which is called oxidative stress, has been recognized to induce cell death.

Cervical cancer is a major cause of cancer-related death in women worldwide and the occurrence of this cancer is ascribed to the changes of genetic and epigenetic events. Epigenetic alterations such as global DNA hypomethylation, hypermethylation of tumor suppressor genes and histone modifications take place during cervical carcinogenesis (15). It was reported that phosphorylated and acetylated forms of histone H3 in cytologic smears are related to the progression of cervical cancer (16). Furthermore, the overexpression of HDAC2 is observed in cervical cancer (17). It has been reported that TSA has anticancer effect in liver, colorectal and breast cancer cells in vitro and in vivo(18–20). However, little is known about the anticancer effect of TSA in cervical cancer cells in view of ROS and GSH levels. Therefore, in the present study, we investigated the effects of TSA on cell growth and death in human cervical HeLa cells in relation to ROS and GSH levels.

Materials and methods

Cell culture

Human cervical adenocarcinoma HeLa cells were obtained from the American Type Culture Collection (ATCC, Manassas, VA) and maintained in a humidified incubator containing 5% CO2 at 37°C. HeLa cells were cultured in RPMI-1640 (Sigma-Aldrich Chemical Co., St. Louis, MO) supplemented with 10% fetal bovine serum (FBS; Sigma-Aldrich) and 1% penicillin-streptomycin (Gibco BRL, Grand Island, NY). Cells were routinely grown in 100-mm plastic tissue culture dishes (Nunc, Roskilde, Denmark) and harvested with a solution of trypsin-EDTA while in a logarithmic phase of growth.

Reagents

TSA was purchased from Cayman Chemical Co. (Ann Arbor, MI) and was dissolved in dimethl sulfoxide (DMSO; Sigma-Aldrich) at 100 mM as a stock solution. The pan-caspase inhibitor (Z-VAD-FMK; benzyloxycarbonyl-Val-Ala-Asp-fluoromethylketone), caspase-3 inhibitor (Z-DEVD-FMK; benzyloxycarbonyl-Asp-Glu-Val-Aspfluoromethylketone), caspase-8 inhibitor (Z-IETD-FMK; benzyloxycarbonyl-Ile-Glu-Thr-Asp-fluoromethylketone) and caspase-9 inhibitor (Z-LEHD-FMK; benzyloxycarbonyl-Leu-Glu-His-Asp-fluoromethylketone) were obtained from R&D Systems, Inc. (Minneapolis, MN) and were dissolved in DMSO at 10 mM to act as stock solutions. NAC was also obtained from Sigma-Aldrich. NAC was dissolved in the buffer [20 mM HEPES (pH 7.0)] at 100 mM as a stock solution. Cells were pretreated with each caspase inhibitor or NAC for 1 h prior to TSA treatment. DMSO (0.05%) was used as a control vehicle.

Growth inhibition assay

Cell growth changes were determined by measuring 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide dye (MTT; Sigma-Aldrich) absorbance in living cells. In brief, 5×103 cells were seeded in 96-well microtiter plates (Nunc) for MTT assays. After exposure to the designated doses of TSA with or without 15 μM of a given caspase inhibitor or 2 mM NAC for the indicated times, 20 μl of MTT solution [2 mg/ml in phosphate-buffered saline (PBS)] were added to each well of 96-well plates. The plates were incubated for 4 additional hours at 37°C. Medium in plates was withdrawn using pipetting and 200 μl DMSO was added to each well to solubilize the formazan crystals. Optical density was measured at 570 nm using a microplate reader (Synergy™ 2, BioTek Instruments Inc., Winooski, VT).

Measurement of HDAC activity

HDAC activity was assessed using the HDAC Assay kit (Millipore, Billerica, MA), according to the manufacturer’s instructions. In brief, 1×106 cells in 60-mm culture dish (Nunc) were incubated with the indicated doses of TSA for 72 h. The cells were then washed in PBS and suspended in 5 volumes of lysis buffer (R&D Systems, Inc.). Protein concentrations were determined using the Bradford method. Supernatant samples containing 20 μg of total protein were used for determination of HDAC activity. These samples were added to each well in 96-well microtiter plates (Nunc) with HDAC substrate provided by the assay kit at 37°C for 1 h. The optical density of each well was measured at 405 nm using a microplate reader (Synergy 2, BioTek Instruments).

Western blot analysis

The expression levels of proteins were evaluated using western blot analysis. In brief, 1×106 cells in 60-mm culture dish (Nunc) were incubated with the designated doses of TSA for 72 h. The cells were then washed in PBS and suspended in 5 vol of lysis buffer (20 mM HEPES. pH 7.9, 20% glycerol, 200 mM KCl, 0.5 mM EDTA, 0.5% NP40, 0.5 mM DTT, 1% protease inhibitor cocktail). Supernatant protein concentrations were determined using the Bradford method. Supernatant samples containing 30 μg total protein were resolved by 10 or 15% SDS-PAGE gels depending on the sizes of target proteins, transferred to Immobilon-P PVDF membranes (Millipore) by electroblotting and then probed with anti-acetylated H3, anti-acetylated H4 (Millipore), anti-Bax (Cell Signaling, Beverly, MA), anti-Bcl-2, anti-PARP, anti-Trx1, anti-Trx2, anti-TrxR1, anti-Cu/Zn SOD, anti-Mn SOD and anti-β-actin antibodies (Santa Cruz Biotechnology, Santa Cruz, CA). Membranes were incubated with horseradish peroxidaseconjugated secondary antibodies. Blots were developed using an ECL kit (Amersham, Arlington Heights, IL). Quantitative data were obtained using an imaging densitometer (ImageJ version 1.33 software, NIH).

Sub-G1 cell analysis

Sub-G1 cells were determined by prop-idium iodide (PI, Sigma-Aldrich; Ex/Em=488/617 nm) staining. In brief, 1×106 cells in 60-mm culture dish (Nunc) were incubated with the designated doses of TSA for 72 h. Cells were then washed with PBS and fixed in 70% ethanol. Cells were washed again with PBS and then incubated with PI (10 μg/ml) with RNase at 37°C for 30 min. The sub-G1 DNA content cells were measured with a FACStar flow cytometer (Becton-Dickinson, San Jose, CA).

Annexin V staining

Apoptotic cell death was determined by staining cells with annexin V-fluorescein isothiocyanate (FITC, Invitrogen Molecular Probes, OR; Ex/Em = 488/519 nm). In brief, 1×106 cells in 60-mm culture dish (Nunc) were incubated with the designated doses of TSA with or without 15 μM of a given caspase inhibitor or 2 mM NAC for 72 h. Cells were washed twice with cold PBS and then resuspended in 500 μl of binding buffer (10 mM HEPES/NaOH pH 7.4, 140 mM NaCl, 2.5 mM CaCl2) at a concentration of 1×106 cells/ml. Annexin V-FITC (5 μl) and PI (1 μg/ml) were then added to these cells. Stained cells with annexin V-FITC were analyzed with a FACStar flow cytometer (Becton-Dickinson).

Quantification of caspase-3 activity

The activity of caspase-3 was assessed using the caspase-3 colorimetric assay kit (R&D Systems). In brief, 1×106 cells in 60 mm culture dish (Nunc) were incubated with 50 nM TSA for 72 h. The cells were then washed in PBS and suspended in 5 vol of lysis buffer provided by the kit. Protein concentrations were determined using the Bradford method. Supernatant samples containing 50 μg of total protein were used for determination of caspase-3 activity. These were added to each well in 96-well microtiter plates (Nunc) with DEVD-pNA as a caspase-3 substrate at 37°C for 1 h. The optical density of each well was measured at 405 nm using a microplate reader (Synergy 2, BioTek Instruments). Caspase-3 activity was expressed in arbitrary absorbance units.

Measurement of MMP (ΔΨm)

MMP (ΔΨm) levels were measured using a rhodamine 123 fluorescent dye (Sigma-Aldrich; Ex/Em=485/535 nm). In brief, 1×106 cells in 60-mm culture dish (Nunc) were incubated with the designated doses of TSA with or without 15 μM of a given caspase inhibitor or 2 mM NAC for 72 h. Cells were washed twice with PBS and incubated with a rhodamine 123 (0.1 μg/ml) at 37°C for 30 min. The cells were washed again twice with PBS and then resuspended in 500 μl of PBS buffer. Rhodamine 123 staining intensity was determined by the flow cytometry (Becton-Dickinson). An absence (−) of rhodamine 123 fluorescence in cells was expressed as the loss of MMP (ΔΨm) in the cells.

Transfection of cells with Bax and Bcl-2 siRNAs

Gene silencing of Bax and Bcl-2 was performed using a siRNA knockdown system. A non-specific control siRNA duplex [5′-CCUACGCC ACCAAUUUCGU(dTdT)-3′], Trx1 siRNA duplex [5′-GCAU GCCAACAUUCCAGUU(dTdT)-3′], Bax siRNA duplex [5′-GCUGGACAUUGGACUUCCU(dTdT)-3′] and Bcl-2 siRNA duplex [5′-CAGAAGUCUGGGAAUCGAU(dTdT)-3′] were purchased from the Bioneer Corp. (Daejeon, South Korea). In brief, 2.5×105 cells in 6-well plates (Nunc) were incubated in RPMI-1640 supplemented with 10% FBS. The next day, cells (∼30–40% confluence) in each well were transfected with the control, Bax or Bcl-2 siRNA [80 pmol in Opti-MEM (Gibco BRL)] using Lipofectamine 2000, according to the manufacturer’s instructions (Invitrogen, Brandford, CT). One day later, cells were treated with or without 100 nM TSA for additional 24 h. The transfected cells were collected and used for western blot analysis, growth inhibition assay, annexin-FITC staining, O2•− and GSH level measurements.

Detection of intracellular O2•− levels

Intracellular O2•− levels were detected by means of an oxidation-sensitive fluorescent probe dye, dihydroethidium (DHE, Invitrogen Molecular Probes; Ex/Em = 518/605 nm). In brief, 1×106 cells in 60-mm culture dish (Nunc) were incubated with the designated doses of TSA with or without 15 μM of a given caspase inhibitor or 2 mM NAC for 72 h. Cells were then washed in PBS and incubated with 20 μM DHE at 37°C for 30 min. The intensity of DHE fluorescence was detected using a FACStar flow cytometer (Becton-Dickinson). O2•− levels were expressed as mean fluorescence intensity (MFI), which was calculated by CellQuest software (Becton-Dickinson).

Detection of intracellular glutathione (GSH) levels

Cellular GSH levels were analyzed using a 5-chloromethylfluorescein diacetate dye (CMFDA, Invitrogen Molecular Probes; Ex/Em = 522/595 nm). In brief, 1×106 cells in 60 mm culture dish (Nunc) were incubated with the designated doses of TSA with or without 15 μM of a given caspase inhibitor or 2 mM NAC for 72 h. Cells were then washed with PBS and incubated with 5 μM CMFDA at 37°C for 30 min. CMF fluorescence intensity was determined using a FACStar flow cytometer (Becton-Dickinson). Negative CMF staining cells indicating GSH depletion were expressed as the percents of (−) CMF cells.

Statistical analysis

The results represent the mean of at least three independent experiments (mean ± SD). The data were analyzed using Instat software (GraphPad Prism4, San Diego, CA). The Student’s t-test or one-way analysis of variance (ANOVA) with post hoc analysis using the Tukey multiple comparison test was used for parametric data. Statistical significance was defined as p<0.05.

Results

Effects of TSA on the growth and HDAC activity in HeLa cells

We first examined the effect of TSA on the growth inhibition of HeLa cells using MTT assays. After exposure to the various concentrations of TSA, HeLa cell growth was dose- and time-dependently decreased with an IC50 of ∼100, 40 and 20 nM at 24, 48 and 72 h, respectively (Fig. 1A). When tested whether TSA as an HDAC inhibitor would inhibit HDAC activity, TSA significantly attenuated the HDAC activity at 72 h (Fig. 1B). Furthermore, it was observed that TSA increased the forms of acetylated histone 3 and 4 in HeLa cells (Fig. 1B).

Figure 1. Effects of TSA on cell growth and HDAC activity in HeLa cells. Exponentially growing cells were treated with the designed concentration of TSA for indicated times. (A) The graph shows cellular growth changes in HeLa cells, as assessed by MTT assay. (B) The graph shows HDAC activity in HeLa cells. The inside figure indicates the levels of acetylated H3 and H4 proteins in TSA-treated HeLa cells. Samples of protein extracts (30 μg) were resolved by SDS-PAGE gel, transferred onto PVDF membranes and immunoblotted with the indicated antibodies against ac-H3, ac-H4 and β-actin. The expression levels of ac-H3 and H4 proteins were quantified using a densitometer, ImageJ software. The relative levels were calculated as the ratio of ac-H3 and ac-H4 to β-actin protein level, respectively. *p<0.05 compared with the control group.

Effects of TSA on cell death and MMP (ΔΨm) in HeLa cells

As shown in Fig. 2A, TSA increased the number of sub-G1 cells in HeLa cells in a dose-dependent manner at 72 h. When HeLa cells were stained with annexin V-FITC to evaluate the induction of apoptosis, the number of annexin V-staining cells in TSA-treated cells was dose-dependently increased (Fig. 2B). In addition, caspase-3 activity was increased in 50 nM TSA-treated HeLa cells (Fig. 2C). Examination of apoptosis-related protein changes during TSA-induced cell death revealed that the levels of Bcl-2 and the intact 116 kDa form of poly(ADP-ribose) polymerase (PARP) were decreased by TSA whereas the level of Bax protein was not strongly altered (Fig. 2C). Moreover, TSA increased the number of MMP (ΔΨm) loss cells in HeLa cells at 72 h in a dose-dependent manner (Fig. 2D).

Figure 2. Effects of TSA on cell death and MMP (ΔΨm) in HeLa cells. Exponentially growing cells were treated with the designed concentrations of TSA for 72 h. (A and B) The graphs show the percents of sub-G1 and annexin V-positive cells, respectively. (C) The graph shows the activity of caspase-3 in samples containing 50 μg of total protein. Western blot analysis shows the levels of Bcl-2, Bax, PARP and β-actin. (D) The graph shows the percents of rhodamine 123-negative [MMP (ΔΨm) loss] cells. *p<0.05 compared with the control group.

Effects of Bax and Bcl-2 siRNAs on cell growth and death in TSA-treated HeLa cells

To investigate the effects of Bax and Bcl-2 on HeLa cell growth and death, HeLa cells were transfected with either non-target control siRNA, Bax or Bcl-2 siRNA. As shown in Fig. 3A, the expressions of Bax and Bcl-2 were clearly decreased by each siRNA as compared with cells transfected with control siRNA. When we observed the effect of Bax or Bcl-2 siRNA on cell growth and death in TSA-treated HeLa cells, Bax siRNA significantly attenuated cell growth inhibition and death by TSA (Fig. 3B and C). On the other hand, Bcl-2 siRNA markedly intensified cell growth inhibition and death in TSA-treated HeLa cells (Fig. 3B and C). In addition, the administration of Bcl-2 siRNA alone induced cell growth inhibition and death in the control HeLa cells (Fig. 3B and C).

Figure 3. Effect of Bax and Bcl-2 siRNAs on cell growth and death in TSA-treated HeLa cells. HeLa cells (∼30–40% confluence) were transfected with non-target control (CTR), Bax or Bcl-2 siRNA. One day later, cells were treated with 100 nM TSA for an additional 24 h. (A) The expressions of Bax and Bcl-2 were examined by western blot analysis. Protein extracts (30 μg) were resolved by SDS-PAGE gel, transferred onto PVDF membranes and immunoblotted with the indicated antibodies against Bax, Bcl-2 and β-actin. (B and C) The graphs show the cell growth (B) and percent of annexin V-positive staining cells (C) in HeLa cells. *p<0.05 compared with the control group. #p<0.05 compared with cells treated with TSA only.

Effects of TSA on intracellular O2•− and GSH levels in HeLa cells

The intracellular O2•− levels were measured in TSA-treated HeLa cells using a DHE fluorescence dye. As shown in Fig. 4A, the O2•− level was significantly increased in TSA-treated HeLa cells at 72 h in a dose-dependent manner. In addition, the level of Mn SOD was upregulated by TSA (Fig. 4B). However, this agent did not strongly influence the levels of other tested antioxidant proteins; Trx1, Trx2, TrxR1 and Cu/Zn SOD (Fig. 4B). In relation to GSH level in TSA-treated HeLa cells, TSA significantly increased GSH depleted cell number at 72 h in a dose-dependent manner (Fig. 4C).

Figure 4. Effects of intracellular O2•− and GSH levels in HeLa cells. Exponentially growing cells were treated with the designed concentrations of TSA for 72 h. The intracellular O2•− and GSH levels were measured using a FACStar flow cytometer. (A) The graph indicates O2•− (DHE) level compared with control cells. (B) Western blot analysis shows the levels of Trx1, Trx2, TrxR1, Cu/Zn SOD, Mn SOD and β-actin. (C) The graph shows the percents of (−) CMF (GSH depleted) cells. *p<0.05 compared with the control group.

Effects of caspase inhibitors on cell growth, death, O2•− and GSH levels in TSA-treated HeLa cells

We determined which caspases were involved in the cell growth inhibition and death of TSA-treated HeLa cells. For this experiment, we chose 50 nM TSA as a suitable dose to differentiate the level of cell growth and death in the presence or absence of each caspase inhibitor; [pan-caspase inhibitor (Z-VAD), caspase-3 inhibitor (Z-DEVD), caspase-8 inhibitor (Z-IETD), or caspase-9 inhibitor (Z-LEHD)]. A concentration of 15 μM caspase inhibitor was used as an optimal dose in this study, this dose did not significantly affect cell death in HeLa control cells. All the caspase inhibitors attenuated cell growth inhibition and death in TSA-treated HeLa cells (Fig. 5A and B). In relation to O2•− and GSH levels, all caspase inhibitors, especially Z-VAD, Z-DEVD and Z-IETD significantly reduced O2•− level in TSA-treated HeLa cells (Fig. 5C). Furthermore, all the caspase inhibitors markedly prevented GSH depletion in TSA-treated HeLa cells (Fig. 5D).

Figure 5. Effects of caspase inhibitors on cell growth, death, O2•− and GSH levels in TSA-treated HeLa cells. Exponentially growing cells were treated with 50 nM TSA and/or 15 μM of a given caspase inhibitor for 72 h. (A and B) The graphs show the cell growth (A) and percent of annexin V-positive cells in HeLa cells (B). (C and D) The graphs indicate O2•− (DHE) levels (C) and the percents of (−) CMF (GSH-depleted) cells (D). *p<0.05 compared with the control group. #p<0.05 compared with cells treated with TSA only.

Effects of NAC on cell growth, death, O2•− and GSH levels in TSA-treated HeLa cells

To investigate the involvement of O2•− level increase in TSA-induced HeLa cell growth inhibition and death, HeLa cells were pretreated with 2 mM NAC as an antioxidant before the treatment of TSA. As shown in Fig. 6A and B, NAC significantly recovered cell growth inhibition and death in TSA-treated HeLa cells. In addition, NAC attenuated the proportion of MMP (ΔΨm) loss cells in TSA-treated HeLa cells (Fig. 6C). When assessed whether NAC influences O2•− and GSH levels, NAC markedly reduced O2•− level and GSH depletion in TSA-treated HeLa cells (Fig. 6D and E).

Figure 6. Effects of NAC on cell growth, death, MMP (ΔΨm), O2•− and GSH levels in TSA-treated HeLa cells. Exponentially growing cells were treated with 50 nM TSA and/or 2 mM NAC for 72 h. (A and B) The graphs show the cell growth (A) and percents of annexin V-positive cells in HeLa cells (B). (C) The graph shows the percents of rhodamine 123-negative [MMP (ΔΨm) loss] cells. (D and E) The graphs indicate DHE (O2•−) levels (D) and the percents of (−) CMF (GSH-depleted) cells (E). *p<0.05 compared with the control group. #p<0.05 compared with cells treated with TSA only.

Discussion

In the present study, we focused on assessing the effects of TSA on cell growth inhibition and death in HeLa cervical cancer cells in relation to ROS and GSH levels. Because TSA decreased the level of HDAC activity and increased the levels of acetylated histones in HeLa cells, TSA seemed to act as an HDAC inhibitor in HeLa cells. This agent remarkably induced the acetylation of histone 4 compared with that of histone 3. However, another hydroxamic acid-derived HDAC inhibitor, SBHA strongly induced the acetylation of histone 3 rather than that of histone 4 in HeLa cells (unpublished data). The different effects of TSA and SBHA on the histone acetylation is probably due to the different functional bioavailability of these hydroxamic acid-derived HDAC inhibitors through various biochemical modifications such as sulfation, hydroxylation, oxidation and methylation in cells. TSA inhibited the growth of HeLa cells in a dose- and time-dependent manner and also induced apoptosis. However, this agent did not significantly induce any specific phase arrest of the cell cycle at 24 and 72 h (data not shown). The growth inhibition in TSA-treated HeLa cells was due to apoptotic cell death rather than a specific cell cycle arrest. TSA dose-dependently triggered the loss of MMP (ΔΨm) and reduced MMP (ΔΨm) levels in HeLa cells (data not shown). The levels of MMP (ΔΨm) loss cells were similar to those of annexin V staining cells (Fig. 2), implying that apoptotic cell death by TSA was tightly correlated with the collapse of MMP (ΔΨm).

A high ratio of Bax to Bcl-2 is known to be the main trigger in the collapse of MMP (ΔΨm) and apoptosis in cells (21). It is reported that HDAC inhibitors downregulate Bcl-2 expression and induce apoptosis in many cancer cells (22,23). Likewise, the level of Bcl-2 protein was downregulated in TSA-treated HeLa cells. Moreover, the administration of Bcl-2 siRNA enhanced the growth inhibition and death of TSA-treated HeLa cells. Therefore, TSA seemed to induce apoptosis in HeLa cells depending on the downregulation of Bcl-2 protein. In relation to Bax protein, TSA did not strongly alter the expression level of Bax protein. However, the administration of Bax siRNA attenuated the growth inhibition and death of TSA-treated HeLa cells. Therefore, these results support the notion that the relatively high ratio of Bax to Bcl-2 can trigger apoptosis in cells. In particular, Bcl-2 siRNA alone induced the growth inhibition and death in HeLa control cells, implying that Bcl-2 protein is a crucial regulator in the survival of HeLa cells. When determined which caspases were involved in apoptosis in TSA-treated HeLa cells, all the tested caspase inhibitors prevented TSA-induced HeLa cell death. In addition, TSA increased the activity of caspase-3 in HeLa cells. Therefore, TSA-induced HeLa apoptosis is mediated by the activation of various caspase cascades. In particular, both cell death receptor pathway of caspase-8 and the mitochondrial pathway of caspase-9 were involved in the induction of apoptosis in HeLa cells.

It is reported that HDAC inhibitor increases ROS levels in solid tumor and leukemia cells (24). Furthermore, oxidative stress seems to be involved in HDAC inhibitor-induced cell death (25). Similarly, the level of O2•− was significantly increased in TSA-treated HeLa cells. Probably, the increased O2•− level mainly resulted from the damage of mitochondria by TSA. Importantly, NAC, which strongly suppressed O2•− levels in TSA-treated HeLa cells, significantly prevented HeLa cell growth inhibition and death by TSA and it also attenuated the collapse of MMP (ΔΨm). In addition, all caspase inhibitors showing the anti-apoptotic effects decreased O2•− levels in these cells. Treatment with Bcl-2 siRNA increased O2•− level in TSA-treated HeLa cells whereas treatment with Bax siRNA decreased the O2•− level in these cells (data not shown). These results suggested that TSA-induced HeLa cell death is mediated by the oxidative stress derived from O2•− level changes.

TSA increased the level of Mn SOD among the various antioxidant proteins in the present study. Mn SOD which is located in mitochondria catalyzes the dismutation of O2•− into oxygen and hydrogen peroxide (26). It is possible that an increase in O2•− level in TSA-treated HeLa cells leads to upregulation of the expression of Mn SOD in a compensatory mechanism. However, the expression level of thioredoxin 2 (Trx2), which is another antioxidant enzyme in mitochondria, was not altered by TSA in HeLa cells. Because it has been reported that DNA methylation and histone modification regulated Mn SOD expression in breast cancer cells (27), it is plausible that the specific upregulation of Mn SOD can be transcriptionally regulated by the inhibition of HDAC by TSA.

GSH as the main cellular non-protein antioxidant can eliminate ROS including O2•−. It is known that the intracellular GSH content has a decisive effect on anticancer drug-induced apoptosis (28,29). According to our current data, TSA increased the number of GSH depleted cells in HeLa cells. All the tested caspase inhibitors and NAC prevented the GSH depletion by TSA. In addition, treatment with Bcl-2 siRNA increased GSH depletion in TSA-treated HeLa cells whereas treatment with Bax siRNA decreased the GSH depletion in these cells (data not shown). Therefore, these results support the notion that apoptotic effects are inversely comparative to GSH content in the cell.

In conclusion, as depicted in Fig. 7, TSA inhibited the growth of HeLa cervical cancer cells via Bcl-2-mediated and caspase-dependent apoptosis, which was closely related to O2•− and GSH content levels.

Figure 7. The diagram for TSA-induced HeLa cell death.

Abbreviations:

Acknowledgements

This study was supported by the Basic Science Research Program through the National Research Foundation of Korea (NRF) funded by the Ministry of Education, Science and Technology (2010-007059) and by a grant from the Ministry of Science & Technology (MoST)/Korea Science & Engineering Foundation (KOSEF) through the Diabetes Research Center at Chonbuk National University (2012-0009323).

References