Research Article | Open Access
Chitra Basu, Runa Sur, "S-Allyl Cysteine Alleviates Hydrogen Peroxide Induced Oxidative Injury and Apoptosis through Upregulation of Akt/Nrf-2/HO-1 Signaling Pathway in HepG2 Cells", BioMed Research International, vol. 2018, Article ID 3169431, 14 pages, 2018. https://doi.org/10.1155/2018/3169431
S-Allyl Cysteine Alleviates Hydrogen Peroxide Induced Oxidative Injury and Apoptosis through Upregulation of Akt/Nrf-2/HO-1 Signaling Pathway in HepG2 Cells
Hydrogen peroxide (H2O2) mediated oxidative stress leading to hepatocyte apoptosis plays a pivotal role in the pathophysiology of several chronic liver diseases. This study demonstrates that S-allyl cysteine (SAC) renders cytoprotective effects on H2O2 induced oxidative damage and apoptosis in HepG2 cells. Cell viability assay showed that SAC protected HepG2 cells from H2O2 induced cytotoxicity. Further, SAC treatment dose dependently inhibited H2O2 induced apoptosis via decreasing the Bax/Bcl-2 ratio, restoring mitochondrial membrane potential (∆), inhibiting mitochondrial cytochrome c release, and inhibiting proteolytic cleavage of caspase-3. SAC protected cells from H2O2 induced oxidative damage by inhibiting reactive oxygen species accumulation and lipid peroxidation. The mechanism underlying the antiapoptotic and antioxidative role of SAC is the induction of the heme oxygenase-1 (HO-1) gene in an NF-E2-related factor-2 (Nrf-2) and Akt dependent manner. Specifically SAC was found to induce the phosphorylation of Akt and enhance the nuclear localization of Nrf-2 in cells. Our results were further confirmed by specific HO-1 gene knockdown studies which clearly demonstrated that HO-1 induction indeed played a key role in SAC mediated inhibition of apoptosis and ROS production in HepG2 cells, thus suggesting a hepatoprotective role of SAC in combating oxidative stress mediated liver diseases.
Oxidative stress in liver hepatocytes underlies various liver diseases . Hydrogen peroxide (H2O2) plays a major role in inducing liver oxidative stress, by disrupting the cellular redox circuitry that depends on the redox state of various signaling molecules behaving as redox sensitive molecular switches, or by directly damaging cellular macromolecules including DNA, proteins, and lipids. This alters many fundamental cellular functions including proliferation, differentiation, migration and adhesion  and eventually results in sustained hepatocyte apoptosis, a pathological condition frequently associated with the progression of several liver diseases such as hepatic ischemia-reperfusion (I/R) injury, alcoholic liver disease, nonalcoholic fatty liver disease, and hepatitis [2, 3].
H2O2 levels that induce oxidative stress have been shown to downregulate heme oxygenase-1 (HO-1), a phase II anti-oxidant enzyme, involved in the rate limiting step of heme metabolism that catalyzes the conversion of heme into carbon monoxide and biliverdin. Several studies have depicted that, induction of HO-1 expression interferes with the progression of a number of hepatic pathophysiological conditions including ischemia/ reperfusion (I/R) injury, liver inflammation, hepatic fibrosis and hepatitis . It has also been shown that HO-1 plays a role in cellular defense mechanism against oxidative stress induced apoptotic cell death [5–7].
S-allyl cysteine (SAC), a potential antioxidant found in the aged garlic extract (AGE) , has been reported to possess cytoprotective effects . SAC has many advantages over other garlic compounds owing to the facts that SAC is odourless and less toxic, pharmacokinetic studies show that it has 98 percent bioavailability , it is the only reliable marker used for studies involving oral garlic intake because it is detectable and increases quantitatively in the blood and it is the only constituent of garlic that does not induce P450 isozymes in the body suggesting that SAC will not cause P450-induced contraindications with drugs .
Several in vivo studies have suggested SAC to protect from oxidative stress induced liver injury. SAC has shown efficacy in protecting from carbon tetrachloride induced liver cirrhosis  and liver injury . SAC improved nonalcoholic fatty liver disease in rats with type 2 diabetes via regulation of hepatic lipogenesis and glucose metabolism . SAC alleviated chromium (VI)-induced hepatotoxicity in rats by inhibiting inflammatory markers . However the detailed mechanism behind the antioxidative and antiapoptotic effects of SAC has not been elucidated. The present study has been designed to investigate the mechanism behind the anti-oxidative and anti-apoptotic potential of SAC in hydrogen peroxide stimulated HepG2 cells, a widely used in vitro model for the study of oxidative injury in liver. For the first time we demonstrate in our study that SAC alleviates hydrogen peroxide induced oxidative injury and apoptosis through upregulation of Akt/Nrf-2/HO-1 signaling pathway in HepG2 cells.
2. Materials and Methods
S-allyl cysteine was purchased from Abcam. Trypan blue, 2′,7′-dichlorodihydrofluorescein diacetate (DCFH2-DA),5,5′,6,6′-tetrachloro-1,1′,3,3′-tetraethyl-imidacarbocyanine iodide (JC-1), and Wortmannin were purchased from Sigma-Aldrich, USA. Dulbecco's modified eagle medium (DMEM), fetal bovine serum (FBS), penicillin-streptomycin, and trypsin-EDTA solutions were purchased from HiMedia, India. INTERFERin siRNA transfection reagent was purchased from Polyplus, USA. Taq polymerase and dNTPs were purchased from Thermo Fisher Scientific, USA. Random hexamer primer and RiboLock RNase inhibitor, and RevertAid reverse transcriptase were purchased from Thermo Scientific, USA. Anti-α-tubulin antibody was purchased from BioBharati LifeScience Pvt. Ltd., India. Anti-Nrf-2, anti-Akt, anti-p-Akt, Bcl2, Bax, caspase 3, and cytochrome c antibodies were purchased from R&D systems, USA. Primers for real time PCR were purchased from Integrated DNA Technologies, USA.
2.2. Cell Culture
HepG2 cells were obtained from National Centre for Cell Science (NCCS), Pune, India, and were cultured in DMEM medium supplemented with 10 % FBS and 1% penicillin-streptomycin at 37°C with 5% CO2.
2.3. Cell Viability Assay
Cell viability was measured using trypan blue exclusion method . Briefly, HepG2 cells were seeded in 24-well plates at a density of 1×105 cells per well for 24 h. Then, dose response and time course experiments were performed with H2O2. Additionally, cells were either left untreated or pre-treated with different concentrations of SAC in the presence or absence of H2O2 for 24 h. Also, cells were either left untreated or treated with H2O2 followed by treatment with SAC (150 μM) for different time points (posttreatment). Then the cells were harvested and trypan blue solution (0.4 %) was added to the cell suspensions in a ratio of 1:1. Finally the numbers of total and dead cells were counted using hemocytometer. The percentage of viable cells was calculated and plotted.
2.4. Cell Cycle Analysis by Flow Cytometry
Cell cycle analysis was performed according to a previously described method . Briefly 4 × 105 cells were seeded in each well of a 6-well plate and incubated for 24 h. Then cells were either left untreated or treated with SAC for 2 h followed by exposure to 1 mM H2O2 for 24 h. Harvested cells were then subjected to chilled 70 % ethanol fixation and RNase A (100 μg/ml) treatment followed by treatment with propidium iodide (120 μg/ml) to stain cellular DNA. The percentages of cells in different phases of the cell cycle were analysed using FACS Verse (Becton–Dickinson) equipped with 405 nm (Violet), 488 nm (Blue) and 640 nm (Red) solid state laser light by acquiring at least 10,000 cells per sample. Data were analyzed using FACSuite software [Version 22.214.171.12442].
2.5. Determination of Apoptosis
Apoptotic cells were detected by Annexin V/PI double staining method. Initially, each well of a 6-well plate was seeded with 4×105 cells and incubated for 24 h. Then cells were either left untreated or pretreated with SAC for 2 h followed by exposure to 1 mM H2O2 in the presence of SAC for 24 h. Cells were subjected to Annexin-V and PI staining with Annexin-V-FLUOS Staining Kit (Roche Diagnostics) according to the manufacturer’s protocol. Finally, the distribution of the apoptotic cells was measured using FACS Verse (Becton Dickinson). The values are represented as fold change over control.
2.6. Measurement of Mitochondrial Membrane Potential
Mitochondrial membrane potential (∆) was measured using the cationic dye JC-1 that accumulates in mitochondria. Initially, each well of a 6-well plate was seeded with 4×105 cells and incubated for 24 h. Then cells were either left untreated or pretreated with SAC for 2 h followed by exposure to 1 mM H2O2 in the presence of SAC for 6 h. Thereafter the cells were washed with PBS followed by staining with 20 μM of JC-1 for 30 min at 37°C. Cells were washed with phosphate buffer saline followed by analysis in FACS Verse. At high concentration (indicative of high ∆) JC-1 accumulates in the intact mitochondria as aggregates yielding red fluorescence (590 nm). However, at low concentration (indicative of low ∆) JC-1 remains predominantly as monomers in the depolarized mitochondria yielding green fluorescence (535 nm) .
2.7. Measurement of ROS Levels
ROS levels were measured by DCFH2-DA staining followed by FACS analysis according to a previously described method . Initially, each well of a 6-well plate was seeded with 4×105 cells and incubated for 24 h. Then cells were either left untreated or pre-treated with SAC for 2 h followed by exposure to 1 mM H2O2 in the presence of SAC for another 2 h. Additionally, cells were pretreated with 1 mM H2O2 followed by SAC treatment or none for different time points. Then cells were stained with 20 μM of DCFH2-DA in serum free media for 30 min at 37°C. DCF fluorescence, an indicator of ROS levels, was measured using FACS Verse.
2.8. Measurement of Lipid Peroxidation
The extent of lipid peroxidation was determined using a previously established protocol . Briefly, HepG2 cells were seeded in 6-well plates at a density of 4×105 and incubated for 24 h. Then cells were either left untreated or pretreated with SAC for 2 h followed by exposure to 1 mM H2O2 for 6 h to stimulate oxidative injury.
After treatment, cells were harvested and lysed by sonicating for 10 sec. Lipid peroxidation was estimated by thiobarbituric acid-reactive substances (TBARS) method  by measuring the levels of malondialdehyde (MDA) produced during cellular lipid peroxidation. In short, the cell lysates were then centrifuged at 10,000 g for 10 min at 4°C. Then equal volume of TBA solution (0.375 % TBA, 15 % trichloroacetic acid, and 0.25 N HCl) was added to the supernatants and heated for 15 min in a boiling water bath followed by centrifugation at 10,000 g for 5 min. Finally absorbance of the supernatant was measured at 535 nm. The values are represented as fold change over control.
2.9. RNA Extraction, Reverse Transcription and Semiquantitative PCR
Cells were seeded in 6-well plates and after treatment; total RNA was isolated using TRIzol reagent (Invitrogen). Equal amount (1.5 μg) of RNA from different samples was subjected to reverse transcription for cDNA synthesis using random hexamer primers, dNTPs, RNase inhibitor, buffer, and reverse transcriptase enzyme. PCR was performed with cDNA as template and gene specific primers for HO-1 and β-actin using Taq DNA polymerase. The primer sequences for human HO-1 gene were 5′-CGGGCCAGCAACAAAGTG-3′ (forward), 5′-AGTGTAAGGACCCATCGGAGAA-3′ (reverse) and primer sequences for human β-actin gene were 5′-CTTCCTTCCTGGGCAT-3′ (forward), and 5′-CAGGGTACATGGTGGTG-3′ (reverse). PCR was performed using the following condition: 94°C for 5 min followed by 35 cycles of 94°C for 30 s, 50°C for 30 s, and 72°C for 30 s, followed by 72°C for 7 min. The amplified products were resolved by 8% polyacrylamide gel electrophoresis and stained with ethidium bromide, and photograph was taken under UV light.
2.10. Protein Extraction and Western Blot Analysis
Whole cell protein extract was prepared by washing the harvested cells with phosphate buffered saline and resuspending the cell pellet in RIPA lysis buffer (50 mM Tris-HCl pH 7.4, 150 mM NaCl, 0.1 % SDS, 1 % NP40, 0.5 % sodium deoxycholate, 0.2 mM Na3VO4, 50 mM NaF, 2 mM EDTA, and protease inhibitor cocktail) for 20 min on ice followed by centrifugation at 13,000 g for 15 min at 4°C. The supernatant was used as whole cell lysate. Cytosolic and nuclear extracts were prepared using a previously described method  with minor modifications. Cells were washed with phosphate buffered saline and centrifuged at 400 g for 10 min at 4°C. The pellet was resuspended in 300 μl cytosolic extraction buffer (10 mM HEPES pH 7.9, 10 mM KCl, 1 mM EDTA, 1 mM EGTA, 1mM DTT, 0.5 mM PMSF, and 0.5 % NP40) containing protease inhibitor cocktail and incubated on ice for 15 min. After rapid mixing for 15 sec followed by centrifugation at 4000 g for 1 min at 4°C, the nuclei were pelleted and the supernatant containing the cytosolic extract was collected. The pellet containing the nuclei was resuspended in 100 μl nuclear extraction buffer (10 mM HEPES pH 7.9, 0.4 M KCl, 1 mM EDTA, 1 mM EGTA, 1mM DTT, 0.5 mM PMSF, 0.5 % NP40, and 20 % glycerol) and vortexed followed by centrifugation at 13,000 g for 15 min at 4°C. The supernatant contained the nuclear extract.
For detection of cytochrome c protein released in the cytosol, cytosolic extract was prepared using a previous method  with few modifications. Briefly cells were washed with phosphate buffered saline and homogenized using homogenization buffer (10 mM HEPES pH 7.4, 250 mM sucrose, 10 mM KCl, 1.5 mM MgCl2, 1 mM EDTA, 1 mM EGTA, 1 mM DTT, and protease inhibitor cocktail) followed by centrifugation at 2000 g for 5 min at 4°C. The supernatant was centrifuged at 13000 g for 25 min at 4°C. The supernatant was used as the cytosolic extract.
Protein concentration in the cell lysates was determined using Lowry’s assay. Equal amount of protein was loaded and separated on SDS-PAGE and transferred to PVDF membrane. The membrane was blocked with 5 % BSA followed by hybridization with respective primary and secondary antibodies. Protein bands were visualized using Luminol reagent (Sigma) and exposing the blot to X-ray film. The image was visualized using gel documentation system (Bio-Rad) and densitometry analysis was performed using Quantity One software. The intensity of protein bands was normalized to their respective internal control.
2.11. Small Interfering RNA (siRNA) Transfection
Predesigned small interfering RNA (siRNA) against HO-1 (sense strand CAGUUGCUGUAGGGCUUUAdTdT) and control siRNA (SR-CL000-005) were purchased from Eurogentec, Belgium. Transient transfection of the siRNA was performed using the INTERFERin transfection reagent according to the manufacturers’ protocol. siRNA transfection was carried out for 72 h.
2.12. Statistical Analysis
All data are expressed as mean ± SD and are representative of at least three independent experiments. P value of < 0.05 was considered significant. Student’s t test was used to assess differences between groups. IC50 value of H2O2 was calculated using KyPlot version 2.0 beta 15 (32 bit).
3.1. SAC Inhibits H2O2-Induced Cytotoxicity in HepG2 Cells
To determine the proper working concentration of H2O2, trypan blue exclusion method was performed with HepG2 cells treated with different doses of H2O2. According to Figure 1(a), H2O2 treatment inhibited HepG2 cell viability in a dose dependent manner. 1 mM cytotoxic dose of H2O2, a concentration below its IC50 value (2 mM), was selected as a standard concentration for subsequent experiments. We also performed a time course experiment with 1 mM H2O2 and found that cell viability gradually decreased with increase in incubation time beginning from 6 h (Figure 1(b)).
In order to determine the cytoprotective concentrations of SAC, HepG2 cells were treated with different concentrations of SAC followed by treatment with H2O2. In the presence of 100, 150 and 200 μM SAC, cell viability increased to 95 ± 1 %, 97 ± 1 % and 98.3 ± 0.6 %, respectively, as compared to the H2O2 treated group (74.3 ± 1.5%) (Figure 1(c)). Higher concentration of SAC (500 μM) decreased cell viability to 81.3 ± 1.5 % when added with H2O2 (Figure 1(c)). Therefore, the cytoprotective concentration of SAC to be used for the subsequent experiments was determined to be between 100 and 200 μM. Next we performed a time course experiment in which we pretreated cells with 1 mM H2O2 for 1 h followed by SAC treatment (150 μM) in the presence of H2O2 for various time-points (Figure 1(d)). We found that 1 mM H2O2 treatment induced cell death in a time dependent manner beginning from 6 h and SAC posttreatment reversed this effect. Interestingly we found that SAC dependent cytoprotection was 6.8 % at 12 h, 22.9 % at 24 h and 30.8 % at 48 h when compared to their respective H2O2 treated control. Thus SAC treatment evoked an increase in cytoprotection compared to control with an increase in time of treatment or an increase in cytotoxicity. To determine whether SAC alone had any effect on cell viability, we treated HepG2 cells with different concentrations of SAC (Figure 1(e)). The tested concentrations of SAC did not affect cell viability up to 200 μM; however low amount of toxicity was observed with 500 μM SAC (value decreased from 100 % to 96 ± 1.8 %).
3.2. SAC Inhibits H2O2-Induced Apoptosis in HepG2 Cells
During acute and chronic liver injury H2O2 triggers hepatocyte apoptosis . To investigate whether the cytoprotective role of SAC against H2O2 induced cytotoxicity in HepG2 cells is mediated via its ability to inhibit apoptosis, cell cycle analysis was performed using propidium iodide (PI) staining followed by flow cytometry. Figure 2(a) demonstrates that H2O2 treatment leads to accumulation of 6.5 ± 1.2 % cells in sub-G1 phase as compared to 2.4 % ± 0.1 % cells in the untreated group. However, we found that this H2O2 induced accumulation of cells in sub-G1 phase decreased (2.6 ± 0.1%) on treatment with 150 μM SAC, indicating that SAC inhibited H2O2 mediated accumulation in sub-G1 phase. N-acetyl cysteine (NAC) was used as a positive control for the experiment.
Apoptosis specific Annexin V and PI double staining assay (Figure 2(b)) demonstrates that a significant (P<0.01) increase in apoptotic cells was observed in H2O2 treated HepG2 cells (3.6 ± 0.7 fold) in comparison to untreated cells. However, SAC treatment dose dependently inhibited H2O2 induced apoptosis and decreased levels to 2.2 ± 0.3 fold for 100 μM and 1.7 ± 0.1 fold for 150 μM of SAC in HepG2 cells. We treated cells with SAC alone (150 μM) and found that SAC showed no significant effect on apoptosis compared to the control (Figure 2(b)).
3.3. SAC Inhibits H2O2 Mediated Increase in Bax/Bcl-2 Ratio, Cytochrome c Release, and Caspase 3 Cleavage in HepG2 Cells
An increase in the ratio of proapoptotic Bax and antiapoptotic Bcl-2 induces mitochondrial cytochrome c release, a hallmark of apoptosis . Release of cytochrome c into the cytosol in turn activates downstream caspases via cleavage, one of which is caspase 3 . We found that H2O2 treatment upregulated Bax and downregulated Bcl-2 expression in HepG2 cells resulting in the increase of Bax/Bcl-2 ratio (4.4 ± 0.5) as compared to the control (1) (Figure 2(c)) and SAC treatment downregulated Bax and upregulated Bcl-2 thus decreasing the Bax/Bcl-2 ratio (1.3 ± 0.4) in comparison to H2O2 treated cells.
In addition, we found that H2O2 treatment increased the cytosolic levels of cytochrome c (3.4 ± 0.5) as compared to the control (1) and SAC treatment decreased these cytosolic levels of cytochrome c (0.4 ± 0.1) (Figure 2(d)). Investigating cleavage of downstream caspase 3 we found that H2O2 treatment increased levels of cleaved caspase 3 (2.8 ± 0.5) compared to control (1) and SAC treatment decreased caspase 3 cleavage (2 ± 0.3) (Figure 2(e)). These results demonstrate that SAC inhibits H2O2 induced apoptosis through modulation of the Bcl-2/Bax dependent cell death pathways. α-Tubulin was used as an internal control.
3.4. SAC Inhibits H2O2 Mediated Decrease of Mitochondrial Membrane Potential () in HepG2 Cells
Release of cytochrome c from mitochondria is closely associated with decrease in mitochondrial membrane potential (∆) . H2O2 has been reported to decrease ∆ in HepG2 cells . In order to investigate the effect of SAC on H2O2 mediated loss of mitochondrial membrane potential (∆) in HepG2 cells, we performed a well-established JC-1 assay followed by flow cytometry. A lower value of aggregate/monomer ratio denotes loss of mitochondrial membrane potential. As indicated in Figure 2(f), H2O2 treatment leads to decrease in aggregate/monomer ratio (10.9 ± 0.43) as compared to the control (18.7 ± 0.49). However SAC treatment increased the aggregate/monomer ratio (13.48 ± 0.14 %, 15.49 ± 1 % for 100 μM, and 150 μM SAC, respectively) in a dose dependent manner as compared to H2O2 treated group. This indicates that SAC restored the H2O2 induced loss of mitochondrial ∆ values. SAC alone showed no significant change in mitochondrial membrane potential over control (Figure 2(f)).
3.5. SAC Inhibits H2O2 Induced Reactive Oxygen Species (ROS) Accumulation in HepG2 Cells
ROS production is by far one of the triggering factors for apoptosis induction . Since SAC is a potent ROS scavenger , we thought of investigating whether SAC inhibits apoptotic cell death via scavenging ROS in H2O2 treated HepG2 cells. First we performed a time course experiment with 1 mM H2O2 and found that 2 h time point showed maximal ROS levels (data not shown). To investigate the effect of SAC on cellular ROS levels, cells were treated with SAC in the presence or absence of H2O2 and ROS accumulation was measured using the well characterized DCFH2-DA fluorescence assay followed by FACS analysis. We would like to mention that the added H2O2 that enters cells and H2O2 dependent further ROS production in cells, contribute to the increase in cellular ROS levels. According to the result (Figure 3(a)), the intensity of DCF fluorescence, which is indicative of the ROS levels, was significantly elevated by 1.7 fold after treatment with 1 mM H2O2 from the ROS levels of the untreated control sample which was set at 1. However, SAC treatment significantly reduced the ROS levels (1.2 fold for 100 μM SAC and 1 fold for 150 μM SAC) in a dose dependent manner. Furthermore, in cells treated with 150 μM SAC alone there was no significant change in ROS levels over control.
To avoid the possibility of SAC scavenging added H2O2 and causing the results in Figure 3(a), we first treated cells with H2O2 for 30 min, washed it off with phosphate buffered saline and then followed by SAC treatment for the indicated time points (Figure 3(b)). SAC was able to significantly inhibit H2O2 induced ROS accumulation in cells when treated for the indicated time points post H2O2 treatment as evident from the fold change in DCF fluorescence of cells treated with both H2O2 and SAC compared to their respective H2O2 treated controls (Figure 3(b)). This experiment clearly demonstrates that SAC is able to scavenge the H2O2 induced ROS accumulation in cells, a hallmark of oxidative stress in cells.
3.6. SAC Inhibits H2O2 Induced Lipid Peroxidation in HepG2 Cells
Excessive ROS levels leads to lipid peroxidation which is indicative of cellular oxidative stress. Lipid peroxidation was estimated via measuring the levels of malondialdehyde (MDA) in cells . The result shows that treatment of HepG2 cells with H2O2 leads to significant increase in MDA levels as a result of increased levels of lipid peroxidation in comparison to the control. However, pretreatment with SAC decreases MDA levels (Figure 3(c)). SAC alone sample showed no significant effect over control on lipid peroxidation in cells.
3.7. SAC Up-Regulates HO-1 in H2O2 Treated HepG2 Cells by Increasing Nuclear Accumulation of Nrf-2 via Akt Phosphorylation
Heme oxygenase-1 (HO-1) is a key endogenous antioxidant enzyme which has been reported to protect cells from oxidative stress induced apoptosis [5, 6] by regulating cellular ROS levels. Thus to elucidate the mechanism underlying SAC’s hepatoprotective role against H2O2 induced oxidative injury in HepG2 cells, we assessed the effect of SAC on HO-1 levels. We find that, H2O2 treatment decreased the mRNA levels of HO-1 and SAC treatment increased these levels (Figure 4(a)). At the protein level, H2O2 treatment down regulated HO-1 and again SAC treatment increased these levels. Treatment with SAC alone has no significant effect on endogenous HO-1 levels (Figure 4(b)).
To elucidate how SAC upregulated HO-1, we assessed the effect of SAC on the nuclear translocation of Nrf-2, the transcriptional regulator of HO-1. Our time course experiment using 1 mM H2O2 revealed that nuclear levels of Nrf-2 decreased with increase in time of H2O2 treatment, with 6 h time point showing maximal reduction in nuclear levels of Nrf-2 over control (Figure 4(c), upper panel) as a consequence of delayed response to oxidative stress [26, 27]. Thus we chose this time point for our experiments. According to Figure 4(d), H2O2 treatment decreased (0.36 ± 0.03) the nuclear levels of Nrf-2 over control (1) and SAC treatment increased Nrf-2 levels in the nuclear extract in H2O2 treated HepG2 cells (0.71 ± 0.04) as compared to the H2O2 treated cells in the absence of SAC (Figure 4(d)). Histone H3 was used as an internal control for nuclear extract and α-tubulin was used as an internal control for cytosolic extract.
Afterwards, we investigated the effects of SAC on Akt phosphorylation, which plays an important role in protecting cells from oxidative injury by modulating the Nrf-2/HO-1 pathway [28–30]. We found that Akt phosphorylation was inhibited by 1 mM H2O2 treatment in a time dependent manner with significant inhibition at 6 hours (Figure 4(c), lower panel). Our result showed that Akt phosphorylation that was inhibited by H2O2 treatment was induced on treatment with SAC. Treatment with SAC alone showed no significant effect on phosphorylated Akt levels from that of control (Figure 4(e)).
To confirm the involvement of SAC mediated Akt phosphorylation on the upregulation of HO-1 protein expression, cells were treated with H2O2 and SAC in the presence of the PI3K inhibitor wortmannin. Akt phosphorylation was inhibited when cells were treated with wortmannin (Figure 4(e), right panel, lane 4). Also, SAC failed to induce Akt phosphorylation in cells treated with wortmannin in the presence of H2O2 (Figure 4(e), right panel, lane 3). Likewise, Figure 4(b) (lane 4) clearly demonstrates that SAC was unable to induce HO-1 expression in cells when Akt phosphorylation was inhibited by wortmannin. From Figure 4(b) it is evident that wortmannin treatment decreased HO-1 protein levels below control. We chose the concentration of wortmannin as 10 μM for our treatments with the intention of inhibiting the basal levels of HO-1 induction in control cells which ensues in these cells due to basal levels of Akt phosphorylation as evident from Figure 4(e) (see controls). Comparison of lane 1 and lane 6 of Figure 4(b) which are without and with wortmannin respectively points out that HO-1 expression in HepG2 cells is regulated via the Akt signaling pathway. Additionally, Figure 4(d) (lane 4) demonstrates that, SAC failed to increase the nuclear levels of Nrf-2 in the presence of wortmannin and H2O2 compared to the SAC and H2O2 treated group in the absence of wortmannin (Figure 4(d), lane 3). These results clearly suggest that SAC upregulates HO-1 via activating the Akt /Nrf-2 pathways.
3.8. SAC Inhibits Apoptosis in H2O2 Stimulated HepG2 Cells by Upregulating HO-1
To directly confirm the involvement of HO-1 in SAC mediated apoptosis inhibition, silencing of HO-1 gene using HO-1 specific siRNA was performed. Transfecting cells with HO-1 specific siRNA significantly reduced HO-1 levels compared to control (Figure 5(a) compare lanes 1 and 6). Additionally we found that when HO-1 specific siRNA transfected cells were treated with SAC and H2O2, SAC failed to upregulate HO-1 levels compared to that in control siRNA transfected cells (Figure 5(a), lanes 4 and 5) in contrast to that in untransfected cells treated with SAC and H2O2 (Figure 5(a), lane 3).
Next, cells transfected with HO-1 siRNA or control siRNA were treated with SAC and H2O2 and subjected to Annexin V and PI staining followed by flow cytometry analysis. As depicted from Figure 5(b), H2O2 treatment increased apoptosis by 4.4 ± 0.12 fold over control which was considered as 1. SAC treatment decreased apoptosis of H2O2 treated cells by 1.7 ± 0.05 fold. Interestingly, SAC failed to inhibit H2O2 induced apoptosis in HO-1 knocked down cells when compared to the control siRNA transfected cells treated with SAC and H2O2 (compare lanes 4 and 5, fold apoptosis 4.5 ± 0.14 and 1.7 ± 0.04, respectively in Figure 5(b)). This result directly indicates that SAC mediated upregulation of HO-1 is responsible for protecting HepG2 cells from H2O2 induced apoptosis.
The involvement of HO-1 induction in regulating mitochondrial membrane potential was demonstrated when HepG2 cells transfected with HO-1 siRNA or control siRNA were treated with SAC and H2O2 and subjected to JC-1 staining. As depicted in Figure 5(c) mitochondrial membrane potential increased after SAC treatment (27 ± 0.9) as compared to H2O2 treated cells (15 ± 1.3). However, treatment with SAC failed to restore ∆ in H2O2 and HO-1 siRNA transfected group in comparison to the control siRNA transfected cells also treated with SAC and H2O2 (compare lanes 4 and 5 in Figure 5(c)). This result suggests that SAC induced restoration of H2O2 mediated loss of ∆ is mediated by increased expression of the antioxidant enzyme HO-1.
3.9. SAC Inhibits ROS Accumulation in H2O2 Induced HepG2 Cells via Up-Regulation of HO-1
To investigate whether the upregulation of HO-1 by SAC is one of the mechanisms by which it decreases ROS levels in cells, HepG2 cells were transfected with HO-1 siRNA before treatment with SAC and H2O2 and then subjected to DCFH2-DA FACS assay. As indicated in Figure 5(d), in untransfected cells treatment with 1 mM H2O2 elevated ROS levels by 1.7 fold compared to the control. SAC treatment significantly reduced H2O2 induced ROS levels to control levels. However, SAC failed to inhibit H2O2 stimulated ROS levels in HO-1 knocked down cells (Figure 5(d), lane 4) compared to control siRNA transfected cells (Figure 5(d), lane 5), suggesting that SAC decreases cellular ROS levels via upregulation of HO-1.
In this work we demonstrated the molecular mechanism by which SAC renders antioxidative and antiapoptotic potential against H2O2 induced cytotoxicity in HepG2 cells. We first determined the cytoprotective effects of SAC in H2O2 treated HepG2 cells. Our results demonstrated that treatment with H2O2 significantly inhibited HepG2 cell viability in a concentration and time dependent manner (Figures 1(a) and 1(b)). SAC pretreatment was found to dose dependently increase cell viability in H2O2 treated HepG2 cells (Figure 1(c)). When cells were first treated with H2O2 followed by SAC treatment (posttreatment), SAC was found to decrease H2O2 induced cytotoxicity at different time points (Figure 1(d)). Interestingly, SAC treatment evoked an increase in cytoprotection compared to control with an increase in time of treatment as well as an increase in cytotoxicity, thus confirming the cytoprotective role of SAC in H2O2 treated HepG2 cells. However, higher concentration of SAC (500 μM) decreased cell viability when added with H2O2 (Figure 1(c)) consistent with the fact that low amount of toxicity was observed with 500 μM SAC treatment alone in HepG2 cells (Figure 1(e)). Since 500 μM SAC treatment induced some amount of toxicity in cells, it was inefficient in reversing the toxic effect of H2O2 compared to lower doses of SAC.
ROS production is an important marker of oxidative stress. SAC has been reported to directly scavenge hydroxyl radical, a byproduct of H2O2 decomposition . In our study we also found that SAC inhibited H2O2 induced ROS accumulation in cells (which includes the added H2O2 that enters cells and the H2O2 induced further ROS production) both when added prior to and post-H2O2 treatment (Figures 3(a) and 3(b)). H2O2 induced ROS production leads to lipid peroxidation, another hallmark of oxidative stress. In our study we found that SAC was able to significantly inhibit H2O2 induced lipid peroxidation (Figure 3(c)) in cells. Since our lipid peroxidation experiment which was performed after 6 h of H2O2 treatment, shows an increase in lipid peroxidation by 3.5-fold which would be possible only via further induced intracellular ROS production (hydroxyl radical and the peroxyl radical cause lipid peroxidation), and since SAC reduced DCF fluorescence post 6 h of H2O2 treatment (Figure 3(b)), we could speculate that SAC scavenges both the added ROS that enters cells and the intracellularly produced ROS in HepG2 cells. Thus we could suggest that the ROS scavenging activity SAC in H2O2 treated HepG2 cells could be one of the mechanisms by which SAC protects cells from oxidative injury.
H2O2 induced ROS production eventually leads to apoptotic cell death in hepatocytes . Figure 2(a) suggests that SAC inhibited H2O2 mediated increase in the sub-G1 peak produced as a result of DNA fragmentation which is an indication of cell death. From Annexin V and PI double staining assay we found that SAC decreased the number of Annexin V positive cells significantly (Figure 2(b)) suggesting that SAC indeed inhibits apoptosis in HepG2 cells. The above results clearly elucidate that SAC exerts antioxidative and antiapoptotic effects in H2O2 induced HepG2 cells.
We evaluated the effect of SAC on the hallmarks of apoptosis such as disruption of mitochondrial membrane potential , release of mitochondrial cytochrome c, alteration in the Bax/Bcl-2 ratio, and proteolytic cleavage of caspase-3. We found that SAC inhibited H2O2 mediated loss of mitochondrial membrane potential (Figure 2(f)), prevented mitochondrial cytochrome c release (Figure 2(d)), decreased the Bax/Bcl-2 ratio (Figure 2(c)), and inhibited caspase-3 cleavage (Figure 2(e)). Thus our results clearly demonstrate that SAC inhibits H2O2 induced apoptosis through modulation of the Bcl-2/Bax dependent cell death pathways.
Next we wanted to determine the molecular mechanism behind the antiapoptotic and antioxidative role of SAC. Various animal studies suggest that SAC protects from oxidative injury via modulation of anti-oxidant enzymes [33–35]. SAC was found to protect hepatocytes from chromium induced hepatotoxicity by decreasing ROS and increasing antioxidant levels . Previous reports demonstrate that upregulation of endogenous HO-1 by cobalt protoporphyrin (CoPP) rescued mice from immune-mediated apoptotic liver damage and prolonged survival . HO-1 induction also protected isolated primary hepatocytes from anti-CD95-induced apoptosis in vitro . Ben-Ari et al. 2013, showed that induction of HO-1 by CoPP protects the liver from apoptosis induced I/R injury. HO-1 induction revealed fewer apoptotic hepatocytes cells, lesser caspase-3 levels, and decreased mean number of proliferating cells (positively stained for Ki67) . Thus, we wanted to determine whether HO-1 was a molecular target of SAC. We first determined whether SAC regulated the expression of HO-1 in HepG2 cells as a protective mechanism against H2O2 induced oxidative injury and apoptosis. For this we assessed the levels of the antioxidant enzyme HO-1 in the presence and absence of SAC. We found that treatment with SAC augmented both the mRNA and protein levels of HO-1 in H2O2 treated HepG2 cells (Figures 4(a) and 4(b)).
In order to identify the mechanism by which SAC upregulates HO-1 expression, we assessed the effects of SAC on the nuclear translocation of Nrf-2, the transcription factor that regulates the expression of HO-1. Nuclear accumulation of Nrf-2 depends on the dose and time of H2O2 exposure to cells. It has been reported that low and moderate (0.125 mmol/L, 0.25 mmol/L, and 0.5 mmol/L) doses of H2O2 exposure of rat pulmonary microvascular endothelial cells led to the nuclear accumulation of Nrf-2, increased transcriptional activity, and induction of ARE-medicated gene expression. In contrast, exposure of cells to high doses of H2O2 (1 mmol/L, 2 mmol/L) led to the nuclear exclusion of Nrf-2, decreased transcriptional activity and downregulation of ARE-mediated gene expression . Jain et al. reported that H2O2 induced Nrf-2 nuclear localization occurs in a time dependent manner in HepG2 cells. After 1 h of 4 mM H2O2 treatment, Nrf-2 translocates to the nucleus as an early response to oxidative stress. However, Nrf-2 was exported out of the nucleus at 4 h after 4 mM H2O2 treatment as a result of delayed response to oxidative stress . For our experiments we used 1 mM H2O2 and treated cells for 6 h, which is a dose and time that exceeds cellular defence mechanisms and mimics a state of cellular oxidative injury and at this dose we have found that Nrf-2 nuclear levels are decreased over control (Figure 4(c), upper panel). Additionally, SAC treatment increased the nuclear translocation of Nrf-2, as evidenced by the comparison of the nuclear levels of Nrf-2 in the H2O2 treated cells in the presence and absence of SAC (Figure 4(d)).
Since the PI3K-Akt signaling pathway has been reported to play important roles in preventing oxidative stress in cells by suppressing apoptosis and promoting cell growth and proliferation via upregulation of HO-1 expression [37–39] in an Nrf-2 dependent manner [28–30], we sought to investigate whether SAC had any effects on the phosphorylation of Akt. In our study, treatment of cells with 1mM concentration of H2O2 mimics high ROS levels that induce apoptosis. Under this scenario we find that Akt phosphorylation is inhibited (Figure 4(e), left panel) which correlates with an induction of apoptosis. Our data is in support of published literature which states that ROS induces apoptosis by inhibiting Akt phosphorylation [30, 40]. Our results show that Akt phosphorylation increased with SAC treatment (Figure 4(e), left panel). We also find that SAC was unable to increase Akt phosphorylation in the presence of the Akt inhibitor wortmannin (Figure 4(e), right panel) which specifically inhibits PI3K, suggesting that SAC probably acts at the level or upstream of PI3K in the pathway. To directly elucidate the involvement of the Akt/Nrf-2 pathway in SAC mediated upregulation of HO-1 expression, HO-1 levels were determined in the presence of wortmannin. SAC was unable to induce HO-1 expression in cells when Akt phosphorylation was inhibited by wortmannin (Figure 4(b)). Also SAC failed to induce the nuclear translocation of Nrf-2 in the presence of wortmannin (Figure 4(d)). Thus we could conclude that SAC upregulated HO-1 in an Akt/Nrf-2 dependent manner. In our SAC alone treated control, we found that SAC failed to increase Akt phosphorylation (Figure 4(e) right panel) and likewise HO-1 expression (Figure 4(b)) over control levels. Since our result demonstrates that SAC regulates HO-1 via Akt phosphorylation only under H2O2 induction, we could speculate that HO-1 induction could be one of the mechanisms via which SAC renders cytoprotection to cells under oxidative stress.
Finally, to corroborate the involvement of SAC mediated upregulation of HO-1 enzyme in protecting HepG2 cells from H2O2 induced apoptosis, we knocked down HO-1 gene using HO-1 specific siRNA. As depicted from Figure 5(b), SAC failed to inhibit H2O2 induced apoptosis in HO-1 knocked down cells as compared to control siRNA transfected cells (Figure 5(b)). Additionally in HO-1 knocked down cells, SAC failed to restore the loss of ∆ in H2O2 treated cells (Figure 5(c), lane 4). This result directly indicates that SAC mediated upregulation of HO-1 is responsible for protecting HepG2 cells from H2O2 induced apoptosis.
Now to investigate whether SAC mediated upregulation of HO-1 is one of the mechanisms by which it decreases ROS levels in cells, we assessed ROS levels in HO-1 knocked down cells in the presence of H2O2 and SAC. We found that ROS levels in HO-1 siRNA transfected cells treated with both H2O2 and SAC (Figure 5(d), lane 4) were higher than the control siRNA transfected cells treated with H2O2 and SAC (Figure 5(d), lane 5). This result points to the involvement of HO-1 in SAC mediated decrease in ROS levels and specifically SAC decreases cellular ROS levels via upregulation of HO-1.
In summary SAC exerts cytoprotective effects reversing H2O2 induced oxidative damage in HepG2 cells. SAC prevents H2O2 induced ROS production, lipid peroxidation, and cellular apoptosis. For the first time we demonstrate that the ROS scavenging activity of SAC via upregulating the antioxidant enzyme HO-1 in an Akt/ Nrf-2 dependent manner is a crucial mechanism underlying the antiapoptotic and antioxidative potential of SAC in HepG2 cells. This work provides valuable insights into the hepatoprotective mechanisms of SAC and portrays a promising therapeutic role of this garlic compound in combating liver oxidative stress and apoptosis which underlie a majority of liver diseases.
The data used to support the findings of this study are included within the article.
Conflicts of Interest
The authors share no conflicts of interest for the publication of this manuscript.
The work was supported by the departmental research grant of the University of Calcutta and DST-FIST facility. Chitra Basu acknowledges University Grant Commission and University of Calcutta for her research fellowship [UGC/307/Fellow (Univ) Dated 7.4.15]. The authors also thank Dr. J. Mukhopadhyay (Bose Institute), Dr. Dipak Dutta (IMTECH, Chandigarh), and Dr. S. Sengupta (Bandyopadhyay) (University of Calcutta) for critically reading the manuscript and comments.
- T. Mello, F. Zanieri, E. Ceni, and A. Galli, “Oxidative stress in the healthy and wounded hepatocyte: a cellular organelles perspective,” Oxidative Medicine and Cellular Longevity, vol. 2016, Article ID 8327410, 15 pages, 2016.
- H. Cichoz-Lach and A. Michalak, “Oxidative stress as a crucial factor in liver diseases,” World Journal of Gastroenterology, vol. 20, no. 25, pp. 8082–8091, 2014.
- L. Cao, X.-B. Quan, W.-J. Zeng, X.-O. Yang, and M.-J. Wang, “Mechanism of hepatocyte apoptosis,” Journal of Cell Death, vol. 9, pp. 19–29, 2016.
- G. Sass, R. Barikbin, and G. Tiegs, “The multiple functions of heme oxygenase-1 in the liver,” Zeitschrift für Gastroenterologie, vol. 50, no. 1, pp. 34–40, 2012.
- B.-W. Lee, S. W. Chun, S. H. Kim et al., “Lithospermic acid B protects beta-cells from cytokine-induced apoptosis by alleviating apoptotic pathways and activating anti-apoptotic pathways of Nrf2-HO-1 and Sirt1,” Toxicology and Applied Pharmacology, vol. 252, no. 1, pp. 47–54, 2011.
- Z. Ben-Ari, Y. Issan, Y. Katz et al., “Induction of heme oxygenase-1 protects mouse liver from apoptotic ischemia/reperfusion injury,” Apoptosis, vol. 18, no. 5, pp. 547–555, 2013.
- J. Busserolles, J. Megías, M. C. Terencio, and M. J. Alcaraz, “Heme oxygenase-1 inhibits apoptosis in Caco-2 cells via activation of Akt pathway,” The International Journal of Biochemistry & Cell Biology, vol. 38, no. 9, pp. 1510–1517, 2006.
- A. L. Colín-González, R. A. Santana, C. A. Silva-Islas, M. E. Chánez-Cárdenas, A. Santamaría, and P. D. Maldonado, “The antioxidant mechanisms underlying the aged garlic extract- and S-allylcysteine-induced protection,” Oxidative Medicine and Cellular Longevity, vol. 2012, Article ID 907162, 16 pages, 2012.
- S. Kodai, S. Takemura, Y. Minamiyama et al., “S-allyl cysteine prevents CC14-induced acute liver injury in rats,” Free Radical Research, vol. 41, no. 4, pp. 489–497, 2007.
- H. Amagase, “Clarifying the real bioactive constituents of garlic,” Journal of Nutrition, vol. 136, no. 3, pp. S716–S725, 2006.
- S. Kodai, S. Takemura, S. Kubo, H. Azuma, and Y. Minamiyama, “Therapeutic administration of an ingredient of agedg-arlic extracts, S-allyl cysteine resolves liver fibrosis established by carbon tetrachloride in rats,” Journal of Clinical Biochemistry and Nutrition, vol. 56, no. 3, pp. 179–185, 2015.
- S. Takemura, Y. Minamiyama, S. Kodai et al., “S-Allyl cysteine improves nonalcoholic fatty liver disease in type 2 diabetes Otsuka Long-Evans Tokushima Fatty rats via regulation of hepatic lipogenesis and glucose metabolism,” Journal of Clinical Biochemistry and Nutrition, vol. 53, no. 2, pp. 94–101, 2013.
- S. K. Anandasadagopan, C. Sundaramoorthy, A. K. Pandurangan, V. Nagarajan, K. Srinivasan, and S. Ganapasam, “S-Allyl cysteine alleviates inflammation by modulating the expression of NF-κB during chromium (VI)-induced hepatotoxicity in rats,” Human & Experimental Toxicology, vol. 36, no. 11, pp. 1186–1200, 2017.
- C. Wang, X. Hu, Y. Gao, and Y. Ji, “ZnO nanoparticles treatment induces apoptosis by increasing intracellular ROS levels in LTEP-a-2 cells,” BioMed Research International, vol. 2015, Article ID 423287, 9 pages, 2015.
- S. Panja, N. B. Ghate, and N. Mandal, “A microalga, Euglena tuba induces apoptosis and suppresses metastasis in human lung and breast carcinoma cells through ROS-mediated regulation of MAPKs,” Cancer Cell International, vol. 16, no. 1, 2016.
- S. Sakamuru, X. Li, M. S. Attene-Ramos et al., “Application of a homogenous membrane potential assay to assess mitochondrial function,” Physiological Genomics, vol. 44, no. 9, pp. 495–503, 2012.
- Y. Kim, Y. Choi, H. Ham, H.-S. Jeong, and J. Lee, “Protective effects of oligomeric and polymeric procyanidin fractions from defatted grape seeds on tert-butyl hydroperoxide-induced oxidative damage in HepG2 cells,” Food Chemistry, vol. 137, no. 1–4, pp. 136–141, 2013.
- S.-M. Lee, Y. Choi, J. Sung, Y. Kim, H.-S. Jeong, and J. Lee, “Protective effects of black rice extracts on oxidative stress induced by tert-butyl hydroperoxide in HepG2 cells,” Preventive Nutrition and Food Science, vol. 19, no. 4, pp. 348–352, 2014.
- R. Sur, D. E. Heck, T. M. Mariano, Y. Jin, W. J. Murphy, and J. D. Laskin, “UVB light suppresses nitric oxide production by murine keratinocytes and macrophages,” Biochemical Pharmacology, vol. 64, no. 10, pp. 1469–1481, 2002.
- J. Jiang, S. Yu, Z. Jiang et al., “N-acetyl-serotonin protects HepG2 cells from oxidative stress injury induced by hydrogen peroxide,” Oxidative Medicine and Cellular Longevity, vol. 2014, Article ID 310504, 15 pages, 2014.
- M. E. Guicciardi and G. J. Gores, “Apoptosis: a mechanism of acute and chronic liver injury,” Gut, vol. 54, no. 7, pp. 1024–1033, 2005.
- A. Basu and S. Haldar, “The relationship between Bcl2, Bax and p53: Consequences for cell cycle progression and cell death,” Molecular Human Reproduction, vol. 4, no. 12, pp. 1099–1109, 1998.
- D. M. Finucane, E. Bossy-Wetzel, N. J. Waterhouse, T. G. Cotter, and D. R. Green, “Bax-induced caspase activation and apoptosis via cytochrome c release from mitochondria is inhibitable by Bcl-xL,” The Journal of Biological Chemistry, vol. 274, no. 4, pp. 2225–2233, 1999.
- E. Gottlieb, S. M. Armour, M. H. Harris, and C. B. Thompson, “Mitochondrial membrane potential regulates matrix configuration and cytochrome c release during apoptosis,” Cell Death & Differentiation, vol. 10, no. 6, pp. 709–717, 2003.
- H.-U. Simon, A. Haj-Yehia, and F. Levi-Schaffer, “Role of reactive oxygen species (ROS) in apoptosis induction,” Apoptosis, vol. 5, no. 5, pp. 415–418, 2000.
- J.-L. Ning, L.-W. Mo, and X.-N. Lai, “Low-and high-dose hydrogen peroxide regulation of transcription factor NF-E2-related factor 2,” Chinese Medical Journal, vol. 123, no. 8, pp. 1063–1069, 2010.
- A. K. Jain and A. K. Jaiswal, “GSK-3β acts upstream of Fyn kinase in regulation of nuclear export and degradation of NF-E2 related factor 2,” The Journal of Biological Chemistry, vol. 282, no. 22, pp. 16502–16510, 2007.
- Y.-J. Jun, M. Lee, T. Shin, N. Yoon, J.-H. Kim, and H.-R. Kim, “Eckol enhances heme oxygenase-1 expression through activation of Nrf2/JNK pathway in HepG2 cells,” Molecules, vol. 19, no. 10, pp. 15638–15652, 2014.
- E.-J. Joung, M.-H. Li, H. G. Lee et al., “Capsaicin induces heme oxygenase-1 expression in HepG2 cells via activation of PI3K-Nrf2 signaling: NAD(P)H:quinone oxidoreductase as a potential target,” Antioxidants & Redox Signaling, vol. 9, no. 12, pp. 2087–2098, 2007.
- Z. Ma, C. Li, Y. Qiao et al., “Safflower yellow B suppresses HepG2 cell injury induced by oxidative stress through the AKT/Nrf2 pathway,” International Journal of Molecular Medicine, vol. 37, no. 3, pp. 603–612, 2016.
- P. D. Maldonado, J. R. Alvarez-Idaboy, A. Aguilar-González et al., “Role of allyl group in the hydroxyl and peroxyl radical scavenging activity of S-allylcysteine,” The Journal of Physical Chemistry B, vol. 115, no. 45, pp. 13408–13417, 2011.
- J. Bai, A. M. Rodriguez, J. A. Melendez, and A. I. Cederbaum, “Overexpression of catalase in cytosolic or mitochondrial compartment protects HepG2 cells against oxidative injury,” The Journal of Biological Chemistry, vol. 274, no. 37, pp. 26217–26224, 1999.
- C.-C. Hsu, C.-N. Huang, Y.-C. Hung, and M.-C. Yin, “Five Cysteine-Containing Compounds Have Antioxidative Activity in Balb/cA Mice,” Journal of Nutrition, vol. 134, no. 1, pp. 149–152, 2004.
- S. Kalayarasan, N. Sriram, A. Sureshkumar, and G. Sudhandiran, “Chromium (VI)-induced oxidative stress and apoptosis is reduced by garlic and its derivative S-allylcysteine through the activation of Nrf2 in the hepatocytes of Wistar rats,” Journal of Applied Toxicology, vol. 28, no. 7, pp. 908–919, 2008.
- A. O. Lawal and E. M. Ellis, “The chemopreventive effects of aged garlic extract against cadmium-induced toxicity,” Environmental Toxicology and Pharmacology, vol. 32, no. 2, pp. 266–274, 2011.
- G. Sass, M. C. P. Soares, K. Yamashita et al., “Heme oxygenase-1 and its reaction product, carbon monoxide, prevent inflammation-related apoptotic liver damage in mice,” Hepatology, vol. 38, no. 4, pp. 909–918, 2003.
- N. Cañas, T. Valero, M. Villarroya et al., “Chondroitin sulfate protects SH-SY5Y cells from oxidative stress by inducing heme oxygenase-1 via phosphatidylinositol 3-kinase/Akt,” The Journal of Pharmacology and Experimental Therapeutics, vol. 323, no. 3, pp. 946–953, 2007.
- M. Salinas, R. Diaz, N. G. Abraham, C. M. R. de Galarreta, and A. Cuadrado, “Nerve growth factor protects against 6-hydroxydopamine-induced oxidative stress by increasing expression of heme oxygenase-1 in a phosphatidylinositol 3-kinase-dependent manner,” The Journal of Biological Chemistry, vol. 278, no. 16, pp. 13898–13904, 2003.
- D. Martin, A. I. Rojo, M. Salinas et al., “Regulation of heme oxygenase-1 expression through the phosphatidylinositol 3-kinase/ Akt pathway and the Nrf2 transcription factor in response to the antioxidant phytochemical carnosol,” The Journal of Biological Chemistry, vol. 279, no. 10, pp. 8919–8929, 2004.
- S. Shin, K. Jing, S. Jeong et al., “The omega-3 polyunsaturated fatty acid DHA induces simultaneous apoptosis and autophagy via mitochondrial ROS-mediated Akt-mTOR signaling in prostate cancer cells expressing mutant p53,” BioMed Research International, vol. 2013, Article ID 568671, 11 pages, 2013.
Copyright © 2018 Chitra Basu and Runa Sur. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.