Modulation of Oxidative Stress: Pharmaceutical and Pharmacological Aspects 2018View this Special Issue
Research Article | Open Access
Simona Anticoli, Donatella Amatore, Paola Matarrese, Marta De Angelis, Anna Teresa Palamara, Lucia Nencioni, Anna Ruggieri, "Counteraction of HCV-Induced Oxidative Stress Concurs to Establish Chronic Infection in Liver Cell Cultures", Oxidative Medicine and Cellular Longevity, vol. 2019, Article ID 6452390, 14 pages, 2019. https://doi.org/10.1155/2019/6452390
Counteraction of HCV-Induced Oxidative Stress Concurs to Establish Chronic Infection in Liver Cell Cultures
Hepatitis C virus (HCV) is a blood-borne pathogen causing acute and chronic hepatitis. A significant number of people chronically infected with HCV develop cirrhosis and/or liver cancer. The pathophysiologic mechanisms of hepatocyte damage associated with chronic HCV infection are not fully understood yet, mainly due to the lack of an in vitro system able to recapitulate the stages of infection in vivo. Several studies underline that HCV virus replication depends on redox-sensitive cellular pathways; in addition, it is known that virus itself induces alterations of the cellular redox state. However, the exact interplay between HCV replication and oxidative stress has not been elucidated. In particular, the role of reduced glutathione (GSH) in HCV replication and infection is still not clear. We set up an in vitro system, based on low m.o.i. of Huh7.5 cell line with a HCV infectious clone (J6/JFH1), that reproduced the acute and persistent phases of HCV infection up to 76 days of culture. We demonstrated that the acute phase of HCV infection is characterized by the elevated levels of reactive oxygen species (ROS) associated in part with an increase of NADPH-oxidase transcripts and activity and a depletion of GSH accompanied by high rates of viral replication and apoptotic cell death. Conversely, the chronic phase is characterized by a reestablishment of reduced environment due to a decreased ROS production and increased GSH content in infected cells that might concur to the establishment of viral persistence. Treatment with the prooxidant auranofin of the persistently infected cultures induced the increase of viral RNA titer, suggesting that a prooxidant state could favor the reactivation of HCV viral replication that in turn caused cell damage and death. Our results suggest that targeting the redox-sensitive host-cells pathways essential for viral replication and/or persistence may represent a promising option for contrasting HCV infection.
Hepatitis C virus (HCV), an RNA virus belonging to the Flaviviridae family, represents a major worldwide concern causing about 400,000 deaths worldwide every year . HCV replication cycle takes place into the cytoplasmic compartment of hepatocyte, and it causes acute or chronic hepatitis. The persistent HCV infection is clinically characterized by lifelong low-level virus production, and it is accompanied by the development of chronic liver infection (in about 80% of infected patients) that can evolve to steatosis, fibrosis, cirrhosis, and in a small percentage (about 20%) of chronically infected patients it can develop to the end-stage hepatocellular carcinoma .
Although the exact molecular mechanisms underlying the HCV-related liver injury are not fully understood, redox alterations of hepatocytes have been extensively described in several chronic liver diseases [3, 4]. Oxidative stress, an imbalance between the reactive oxygen species (ROS) production and their clearance by scavenging molecules, has been recognized as a leading factor in inducing hepatocyte death, inflammation, and fibrogenesis, which are responsible for induction and perpetuation of liver damage . Several authors report a rise of ROS levels during HCV infection [6–13], and various viral proteins are known to induce and/or augment the ROS production, including HCV core, E1, E2, nonstructural (NS) 3, NS4B, and NS5A [11, 14–17]. Moreover, the simultaneous induction of several ROS-producing pathways and enzymes, such as the endoplasmic reticulum (ER) oxidoreductases [15, 18] and NADPH (nicotinamide adenine dinucleotide phosphate) oxidases (NOXs) [15, 16, 19], also contributes to HCV-induced oxidative stress. On the contrary, other studies report an increase in the antioxidant defenses, such as superoxide dismutase (SOD), peroxiredoxin (PRDX), glutathione S-transferase (GST) enzyme activity, and GSH levels [14, 20–23]. Glutathione is an important radical scavenger that directly and indirectly neutralizes a variety of reactive molecules, such as superoxide anions (O2⋅−), hydroxyl radicals, and hydrogen peroxide (H2O2) . The ratio between reduced (GSH) and oxidized (GSSG) form of GSH is considered an important indicator of the antioxidant capacity of the cell. Conflicting results are shown about the effect of HCV on intracellular GSH metabolism [17, 19, 23, 25–27]. Indeed, Roe and collaborators  report a significant raise of GSSG in HCV-infected cells, while increased GSH concentration has been demonstrated by de Mochel et al.  using the same in vitro infection system. Interestingly, Abdalla et al.  describe the different effects of two viral proteins on cell antioxidant defenses. In fact, hepatocytes overexpressing HCV core protein have reduced GSH levels and increased the oxidation of thioredoxin (Trx), while the overexpression of viral NS5A protein (known for its ability to cause oxidative stress)  increases antioxidant enzymes (MnSOD and catalase), heme oxygenase-1 (HO-1), and GSH content. Finally, patients with chronic hepatitis C show a depletion of GSH content, which increases after antioxidant treatment . However, different genotypes of HCV exhibit different abilities to induce oxidative stress . In fact, in patients chronically infected with genotype 1a/b, a sharp decrease of reduced GSH level has been observed with respect to the other genotypes, suggesting the more serious disease associated with this genotype .
Interestingly, the de novo synthesis of GSH is controlled by the transcription factor Nrf2 (NF-E2-related factor 2), which regulates the expression of cytoprotective genes. Some studies demonstrate that acute HCV infection is associated with an early induction of proteins functioning in cellular stress responses, including the Nrf2-mediated oxidative stress response [23, 25]. On the other hand, HCV core impairs the Nrf2/ARE signaling pathway by inducing the translocation of sMaf proteins in the cytoplasm, where they bind to NS3 as part of the replication complex. As a result, Nrf2 is trapped in the cytoplasm and is unable to function as transcription factor [26, 30].
On the basis of the conflicting results reported in the literature about the relationship between redox balance and HCV infection, the goal of this study was to clarify whether the virus is able to condition the redox environment of infected cells in order to induce acute infection or to establish its persistence into the cells. For this reason, we set up an in vitro system that mimics as closely as possible the acute and chronic HCV infection.
Here, we demonstrate that during the acute phase of infection HCV replicates with a high rate, thus inducing intense apoptosis in infected cells; in this phase, a marked oxidative stress was registered mainly due to NOX4 activity and to a decrease of GSH and consequently of GSH/GSSG ratio. Conversely, during the chronic phase of infection, low level of both HCV replication and apoptosis was observed, ROS production returned to basal level, GSH content was reestablished, and the GSH/GSSG ratio shifted versus the reduced form of GSH. Moreover, the treatment of HCV-chronically infected cells with a prooxidant drug, auranofin, was able to reactivate viral replication.
2. Materials and Methods
2.1. Cell Lines
Huh-7.5 human hepatoma cells were generously provided by Dr. Charles M. Rice . Cells were grown in high-glucose Dulbecco’s modified Eagle’s medium (DMEM) (Sigma) supplemented with 100 U/ml of penicillin, 100 μg/ml of streptomycin, nonessential amino acids, and 10% fetal bovine serum (FBS) (Invitrogen) at 37°C in 5% CO2.
The virus stock used in this study was prepared as described below. The FL-J6/JFH1-5’C19RLuc 2Ubi plasmid, encoding the entire viral genome of a chimeric strain of HCV genotype 2a, J6/JFH1 , was kindly provided by C. M. Rice. The plasmid was linearized by XbaI digestion and treated with mung bean nuclease to remove 5 end overhangs. The linearized DNA templates were first purified by phenol:chloroform extraction and ethanol precipitation and then transcribed with T7 RNA polymerase using a MEGAscript™ T7 kit (Ambion, Austin, TX) according to the manufacturer’s protocol. For electroporation, Huh-7.5 cells were grown to 60–80% confluence, trypsinized, washed twice in cold PBS, and resuspended in cold PBS at a concentration of cells/ml. 0.4 ml aliquots were mixed with 10 μg of in vitro transcribed RNA and dispensed into 0.4 cm Gene Pulser cuvettes (Bio-Rad). Samples were pulsed using a Gene Pulser apparatus (Bio-Rad, Hercules, CA) with a single pulse at 0.27 kV and 960 mF. Cells were resuspended in 20 ml of complete growth medium, plated and incubated at 37°C, 5% CO2, and 100% relative humidity. Cells were splitted every 3 days, and virus infectivity was measured by immunofluorescence assay as described below and expressed as TCDI50/ml. The culture supernatant from the 4th passage was used to infect naïve Huh-7.5 cells at a multiplicity of infection (m.o.i.) of 0.2 in serum-free high-glucose DMEM. After 2 hours at 37°C, the medium was removed and replaced with complete medium. After 7 days and 2 passages, the supernatants were collected, centrifuged at 1200 rpm for 10 min at 4°C, cleared of debris through filtration on 0.45 μm pore size filters, and stored at -80°C as virus stocks.
2.3. Cell Infection and Viral Titer Assays
Huh7.5 cells were plated, grown for 24 h, and then challenged with virus stock in serum-free medium at 0.01 m.o.i. Culture supernatants of uninfected cells served as a control (mock preparation). Cells were incubated in the presence of the virus for 6 h at 37°C. After the viral challenge, mock-infected and virus-infected cells were washed with PBS and then cultured with fresh medium containing 10% FBS.
The titer of infectious HCV was determined by the 50% tissue culture infective dose (TCID50) assay. Cell supernatants were serially diluted 10-fold in complete DMEM and used to infect 1 × 104/well naïve Huh-7.5 cells in 96-well plates (8 wells per dilution). The level of HCV infection was determined three days postinfection by immunofluorescence staining for HCV core protein. The wells showing positive staining for HCV core protein were counted, and the TCID50 titer was interpolated using the Reed-Muench method .
2.4. Cell Treatments
Auranofin was obtained from Sigma-Aldrich (Heidelberg, Germany). The compound was dissolved in dimethylsulfoxide (DMSO) and applied to the cells at a final concentration of 200 nM that is the concentration at which no toxic effects were observed. The highest DMSO concentration present in the culture medium was 0.05%. Control cells were treated with an equivalent concentration of vehicle.
2.5. Cytotoxicity Assay
Cytotoxicity of auranofin was determined by cell count, and cell viability was assessed by trypan blue dye exclusion test.
2.6. Immunofluorescence Assay
Cells were fixed in methanol : acetone (50 : 50, V/V) for 20 min at -20°C. After blocking with PBS containing 1% bovine serum albumin (BSA) for at least 30 min, cells were incubated with mouse monoclonal antihepatitis C virus core 1b antibody (Abcam, AB 58713); bound antibodies were revealed with mouse anti-human IgG conjugated with Alexa Fluor 488 (Life Technologies, Z25102). After washing, the nuclei were stained with 1 μg/ml 4,6-diamidino-2-phenylindole (DAPI; Molecular Probes) in PBS for 15 min at room temperature. Fluorescent images were acquired on an Olympus IX70 microscope equipped with Nanomover and softWoRx DeltaVision image acquisition software (Applied Precision, WA, USA) and a U-PLAN-APO 40× objective. Images were captured under constant exposure time, gain, and offset.
2.7. Western Blotting
Cells were detached, washed with cold PBS, and centrifuged at 700 g for 10 min. The pellet was lysed in cold RIPA lysis buffer (20 mM TRIS pH 8, 150 mM NaCl, 1% Triton-X 100, 0.1% SDS, 1% sodium deoxycholate) containing protease and phosphatase inhibitors for 30 min on ice. Lysates were centrifuged at 10 000 g for 30 min at 4°C to remove debris.
Protein concentration of cell extracts was determined by the Bradford method (Bio-Rad, 5000006). Lysates were resolved by SDS-PAGE and blotted onto nitrocellulose membranes. The membranes were blocked with 10% nonfat dry milk in Tris-buffered saline containing 0.01% Tween-100 for 1 h at room temperature (RT) and then incubated with specific primary antibodies used at final concentration of 1 μg/ml. The antibodies used are as follows: rabbit polyclonal anti-NOX4 (Santa Cruz Biotechnology, sc-30141), rabbit polyclonal anti-NOX1 (Abcam, ab55831), rabbit monoclonal anti-Nrf2 (D1Z9C) (Cell Signaling Technology, Euroclone, Pero (MI) Italy, 12721S), mouse monoclonal antitubulin (Sigma-Aldrich, T5168), and mouse monoclonal anti-Lamin A/C (Sigma-Aldrich, L1293). Immunocomplexes were detected through peroxidase-coupled secondary antibodies (Jackson), followed by enhanced chemiluminescence (GE Healthcare Life Sciences). Densitometry was done using Quantity One 1-D Analysis software (Bio-Rad).
2.8. Glutathione Assay
The measurement of total intracellular glutathione (tGSH) (including the reduced and oxidized forms, GSH and GSSG, respectively) and GSSG was performed by means of Cayman’s GSH assay kit (Cayman Chemical Co., 703002) according to the manufacturer’s instructions. Briefly, the confluent control and infected Huh7.5 cells were washed twice with PBS, harvested using a rubber policeman, and were homogenized by a freeze-thaw method in 1 ml of 50 mM MES buffer pH 6 containing 1 mM EDTA. After centrifugation, a small amount of the supernatant was used for the protein assay (Bio-Rad protein assay). The residual supernatant was deproteinated by adding an equal amount of 5% w/v of metaphosphoric acid. After centrifugation (at 3000 ×g for 5 min), the supernatant was neutralized with 50 μL of triethanolamine per ml of sample. The tGSH level was then determined by the endpoint method reading absorbance at 405 nm after 25 min, according to the procedures recommended by the manufacturer. In another experiment, GSH was masked by 2-vinylpyridine for 1 h before the assay to determine the GSSG levels in the samples. The tGSH and GSSG were determined by comparison with standards, normalized to protein content, and expressed as nmol/mg protein. The GSH content was obtained by subtracting the GSSG from the tGSH.
2.9. Cell Death Determination
The quantitative evaluation of apoptosis was performed by a double-staining flow cytometry method using fluorescein isothiocyanate- (FITC-) conjugated annexin V(AV)/propidium iodide (PI) apoptosis detection kit (Marine Biological Laboratory, MBL, Woods Hole, MA, USA), according to the manufacturer’s protocol, which allows discrimination among early apoptotic, late apoptotic, and necrotic cells.
2.10. ROS Assay
ROS production was determined by means of the CellROX deep red reagent (Thermo Fisher, C10491), which is a fluorogenic probe, as described in the manufacturer’s instructions. CellROX (5 μM) was added to cell cultures and incubated at 37°C for 30 minutes. Then cells were fixed with paraformaldehyde (4%), and samples were immediately analyzed with an LRS II cytometer (Becton Dickinson, San Jose, CA, USA) equipped with a 488 argon laser and a UVB laser. The data obtained were analyzed by DIVA software (B&D). The median values of fluorescence intensity histograms were used to provide a semiquantitative assessment of ROS production. Samples were acquired with a FACScalibur cytometer (BD Biosciences) equipped with a 488 argon laser and with a 635 red diode laser. At least 20,000 events were acquired. Data were recorded and statistically analyzed by a Macintosh computer using CellQuest software (BD Biosciences). The median values of fluorescence intensity histograms were used to provide a semiquantitative assessment of ROS production.
2.11. Real-Time RT-PCR Analysis
Total RNA was isolated from control and HCV-infected cells, harvested at the indicated times p.i., with the RNeasy kit (Qiagen, 74104) according to the manufacturer’s instructions. Isolated RNA (1 μg) was reverse transcribed to cDNA using iScript™ cDNA Synthesis Kit (Bio-Rad, 1708890). A comparative real-time PCR analysis of gene expression was performed with the iQ™ SYBR Green Supermix (Bio-Rad, 170-8880) and analyzed on LightCycler iQ™ 5 (Bio-Rad). The following forward and reverse primers were used: NOX4 (5-CAGGAGAACCAGGAGATTGTTG-3 forward; 5-GAAGTTGAGGGCATTCACCAGATG-3 reverse), GR (5-TTCAGTTGGCATGTCATC-3 forward; 5-CCGTGGATAATTTCTATGTGA-3 reverse), GS (5-GTGCTACTGATTGCTCAA-3 forward; 5-ACATGGATCTTCCTGTCT-3 reverse), GCL (5-AAGTCCCTCTTCTTTCCA-3 forward; 5-CCTTGAATATTGGCACATTG reverse), and GAPDH (5-TGCGACTTCAACAGCAACTC-3 forward; 5-ATGTAGGCCATGAGGTCCAC-3 reverse).
The housekeeping glyceraldehyde-3-phosphate dehydrogenase (GAPDH) was used for normalization. Relative quantitative evaluation was performed by the comparative ΔΔCt method. The results are presented as fold increase relative to control cells. Dissociation curves were generated to ensure a single amplicon had been produced.
The production of intracellular viral RNA was assessed by quantitative one-step RT-PCR carried out using an ABI 7000 Real-Time PCR System (Applied Biosystems). 5 μl of total RNA was mixed with 2x TaqMan One-Step RT-PCR Master Mix (ABI) and 1 μM forward (TCCCGGGAGAGCCATAGT), 1 μM reverse primers (CCCAGTCTTCCCGGCAATT), and 200 nM probe (FAM- CACCGGTTCCGCAGACC -TAMRA). In vitro transcribed genotype 2a RNA was used as a standard to quantify the copy numbers of viral RNA.
2.12. Data Analysis and Statistics
A statistical significance was evaluated using GraphPad Prism™ (San Diego, CA, USA) software version 6.0. All data reported were verified in at least 3 independent experiments and are reported as deviation (SD). Test details of each experiment are described in the figure legends. values < 0.05 were considered significant.
3.1. Generation of an In Vitro Model of Acute and Chronic HCV Infection
In the attempt to set up an HCV infectious cell culture system that mimics acute and chronic HCV infection, human hepatocellular carcinoma cell line (Huh7.5) was infected with HCV at low (0.01) m.o.i. to allow a multiple-cycle replication, as described in Materials and Methods, and cultured up to 76 days.
After viral adsorption, cell culture viability was monitored at different time points, and viral replication was evaluated by both real-time RT-PCR and immunofluorescence assay for HCV core protein.
The number of viral core positive cells was estimated by immunofluorescence to evaluate the extension of HCV-infected cells. During the first two passages (8 days postinfection), about 80% of the cells were stained for HCV core protein, thus indicating a high rate of HCV replication corresponding to the “acute” phase of infection (Figure 1(a) left side). On the contrary, in the late stage of infection (76 days postinfection p.i.), here referred as the “chronic” phase, only about 15% of the cells expressed the core protein (Figure 1(a) right side). Similarly, the HCV RNA in intracellular compartment reached the highest titer ( copies/μg total RNA vs. p0) 8 days p.i., and it decreased after the recovery phase of the cell culture and during the chronic phase (/μg total RNA at 44 days p.i and copies/μg total RNA at 76 days p.i.) (Figure 1(b)) that is consistent with a persistently infected cell culture. Furthermore, in correspondence with the maximum titer of HCV RNA, the number of HCV-infected cells was significantly reduced compared to uninfected ones (Figure 1(c)). In fact, trypan blue dye exclusion assay showed a significant decrease of alive cells during the so-called “crisis” phase that lasted about two weeks during which the infected cultures were not splitted. Particularly, on days 8 and 14 most of the cells became rounded, detached from the plate, and floated in the culture medium (data not shown). Furthermore, FACS analysis of annexin V/PI double staining of cells showed that infected cells underwent apoptotic death only during the crisis phase. In fact, as shown in Figure 1(d) (right panel), the percentage of double-stained PI+/AV+ cells increased with respect to uninfected cells (CTR) at passage 2 (p2). The 5-fold increase in percentage of apoptotic cells (obtained as mean from 4 independent experiments) was detected in infected cultures at 14 days p.i., compared to the uninfected ones (Figure 1(d), right panel). Interestingly, apoptotic death in infected cell cultures coincided with the highest intracellular viral RNA titer (Figure 1(b)), thus suggesting a causative link between the rate of HCV replication and cell death. Subsequently to the crisis phase, cells started a recovery phase at the end of which the number of live cells, in HCV-infected cultures, was comparable to that of control cells (Figure 1(c); see value at p4). Accordingly, FACS analysis demonstrated that from 37 days p.i. up to 76 days p.i., the percentage of apoptotic cells returned to control values upon recovery of the cultures (Figure 1(d) right panel; see values at p4, p6, p13, and p18). Moreover, from this time point up to 76 days p.i. (chronic phase), the percentage of HCV core-positive cells decreased to 15% (Figure 1(a) right panel) vs. 80% of the acute phase, thus mirroring viral titer trend (see Figure 1(b)). These results strongly suggested a steady state level of HCV replication.
Collectively, the results demonstrate that initial infection of Huh7.5 cells with low m.o.i. leads to obtain an acute in vitro infection featured by apoptotic death of infected cells, here named “acute phase”. This latter is followed by the recovery of the infected cell cultures characterized by lower virus replication and subsequently by the establishment of a persistent infection, here named “chronic phase”. All these characteristics indicated that an in vitro model of persistent infection with Jc1-HCV was set up.
3.2. HCV Infection Increases ROS Production through NOX4 and NOX1 Activity
Redox changes, in particular increased ROS levels, had been associated with HCV infection [34, 35]. Nevertheless, the impact of intracellular HCV replication on cellular redox environment is so far contradictory. To this aim, confluent monolayers of Huh7.5 cells were infected with HCV, and at different time points after viral adsorption, ROS production was measured through FACS using the ROS-sensitive probe CellROX. As shown in Figure 2(a), a significant increase in intracellular ROS levels (more than 3 times higher compared to control) was detected in infected cells 8 days p.i. (p2), when HCV RNA reached the maximum value, and was maintained at high levels during all the apoptotic crisis period. After cell cultures recovery from 37 up to 76 days p.i., the ROS levels in infected cells returned to control values (Figure 2(a) right panel). These results suggest that intracellular ROS-mediated oxidative stress was induced by HCV replication, and it was simultaneously accompanied by the apoptotic phase.
Next, we investigated whether in our model the increase of ROS levels was associated with NOXs activity, particularly with two isoforms, NOX1 and NOX4, involved in the severity of HCV infection [19, 36]. To this aim, Huh7.5 cells were infected with HCV and assayed for NOX4 mRNA by RT-PCR during the different phases of HCV infection. The results demonstrated that the NOX4 mRNA levels doubled 6 days p.i. (p1) in infected cells with respect to uninfected control cells; then the NOX4 mRNA levels decreased and returned to physiological level (Figure 2(b)). Consistently, NOX4 protein expression was upregulated in infected cells during the acute phase, while it was decreased during the chronic phase (Figure 2(c)). Similar results were obtained for NOX1 enzyme, although its decrease began earlier (p3) than NOX4.
Collectively, these data suggest NOX enzymes as one possible player in HCV-induced ROS production.
3.3. HCV Alters the GSH Redox Homeostasis
To test whether Huh7.5 cells activated GSH antioxidant system in response to HCV-induced oxidative stress, the intracellular content of both reduced (GSH) and oxidized (GSSG) forms of glutathione was measured at different times after HCV infection by using a colorimetric assay. As shown in Figure 3(a), in the early steps of acute phase of infection GSH content diminished of about 40% (, at 2 (p0) and 6 (p1) days p.i, respectively) compared to uninfected cells. In contrast, the GSH levels in infected cells were significantly higher (about 70%) during cell recovery (p3) compared to the control cells and were maintained at higher levels during the chronic phase (p4, p5, and p10). More interestingly, by comparing the acute and chronic phases, a significant rise trend of GSH content in infected cells was detected in the latter phases (p3, p4, and p5 vs. p0). Conversely, as shown in Figure 3(b), the GSSG levels increased during the acute phase, in particular the content was doubled 8 days p.i. (p2). Interestingly, as shown in Figure 3(c), the GSH/GSSG ratio that under physiological conditions is maintained >1  was shifted toward the oxidized form and was <1 (p1 and p2), just when viral replication reached the peak (Figure 1(b)), while during the chronic phase the ratio was >1, indicating a restore of physiological redox environment.
Intracellular GSH is regenerated from the oxidized form by glutathione reductase (GR) or synthesized ex novo by the consecutive actions of glutamate cysteine ligase (GCL) and GSH synthase (GS) . Therefore, we evaluated the transcriptional expression of these 3 enzymes both during the acute and chronic phase of infection. As shown in Figure 4(a), the mRNA levels of GR were strongly upregulated during the early steps of infection (p1 and p2), when the GSSG levels were high, while GCL and GS enzyme expression increased starting from the end of acute phase until the recovery period and when the peak of GSH content (p3) was detected. Interestingly, these enzymes were still activated during the chronic phase (p4), suggesting the necessity to maintain a reduced environment in long-term cultures.
Finally, we decided to evaluate whether these enzymes were under the control of Nrf2 pathway. Therefore, we analyzed Nrf2 protein expression during both the acute and chronic phases. As shown in Figure 4(b), Nrf2 seemed to be downregulated by the virus in the early phases of infection, while it was more expressed late in infection, at p4 and p10 when the chronic phase was well-established.
All these results suggest that oxidative stress during the acute phase is useful for promoting viral replication, while the reducing conditions observed in the chronic phase probably favor viral persistence into the cells.
3.4. Auranofin-Induced Oxidative Stress Leads to Increased Levels of HCV RNA Copies
Since the intracellular redox conditions seem to play a key role in the establishment of the chronic phase of HCV infection, we decided to evaluate whether the oxidative stress could reactivate HCV replication in chronically infected cells. For this reason, a chemical treatment with auranofin (Au), a well-known prooxidant drug  that induces ROS production in infected cells [40, 41], was used. In our experimental model, treatment with Au (200 nM) for 48 hrs was able to induce an increment of intracellular ROS levels by twofold, either in uninfected (CTR) or in HCV-infected cells (Figure 5(a)). In parallel, the number of intracellular HCV RNA copies in Au-treated cultures was about 40% greater than that of untreated infected cells (Figure 5(b)). Interestingly, in this condition, only HCV-infected cell cultures underwent apoptosis (Figure 5(c)), suggesting that oxidative stress induction could favor viral replication that in turn caused cell damage and death.
Oxidative stress has emerged as a key contributor to the development and progression of HCV-induced pathogenesis of liver [34, 35, 42] and the associated development of hepatocellular carcinoma . The lack of an in vitro system that recapitulates the different stages of HCV chronic infection has hampered the disclosure of the exact mechanisms and the mutual effect of HCV infection and oxidative stress pathways on the host cells. In this study, we were able to set up the HCV infectious system in Huh7.5 cells, which are permissive to the JFH1 infectious clone . Particularly, infection of cell monolayers with low m.o.i. of HCV allowed to obtain first an acute infection and subsequently the establishment of a persistent infection. We demonstrated that, during the acute phase, high percentage of infected cells underwent apoptosis and viral titer peaked, whereas during the chronic phase viral replication was reduced and consequently the percentage of apoptotic-infected cells. This model called “long-term infected cultures” (LTIC) could mimic the same stages of a natural HCV infection. It is interesting that HCV has long been believed noncytopathic virus, and the hepatocyte damage during infection was considered to be mediated by the immune system. However, consistent with previously reported results , we could demonstrate that HCV induces cell death during in vitro infection of Huh7.5 cells in the absence of RIG-I-mediated innate immune response. The presence of low number of core expressing cells, during the here called “chronic phase”, paralleled by the low level viral RNA titer, indicated the ability of the JFH1 clone of HCV to persistently infect susceptible cell cultures. With regard to the mechanisms involved in establishing in vitro persistence, there could be a close virus-host cell interaction, and as reported by Zhong et al. , in Huh7.5 cells long-term infected by HCV, some cells resistant to reinfection, due to the loss of HCV receptor CD81, can be selected during the chronic phase. From the virus side, HCV is known to exist as quasispecies in patients in vivo, and during persistent infection in vitro, some virus variants can arise that are more adapted in cultures and able to persist without killing the host cells or having reduced infectivity . These points will deserve deeper investigation in the future.
Furthermore, during HCV acute infection, a ROS overproduction, mainly mediated by NADPH-oxidase NOX4, was registered in infected cells. NOXs are a family of seven enzymes, generating O2⋅− or H2O2 from molecular oxygen . Accumulating evidence indicates that NOX-mediated ROS production has a critical role in hepatic fibrosis [46, 47], and in particular, NOX4 is involved in the severity of HCV-associated liver disease [19, 36], as well as in the regulation of viral replication of different viruses [48–50]. Here, we found that NOX4 and NOX1 rise mirrored the trend of ROS production and that of viral replication; in fact, their expression was increased during the acute phase of infection, while it decreased late in infection, thus suggesting a critical role for NOXs also in regulating HCV replication cycle. The reason why both NOX enzymes were downmodulated in infected cells during the chronic phase is still unclear, but we hypothesize that it could be a further mechanism induced by the virus to maintain reducing environment into host cell for the establishment of its persistence. Indeed, other viruses are able at the same time to positively and negatively modulate NOX isoforms to their advantage [48–50]. Further studies will be needed to clarify this aspect.
It is noteworthy that NOX4 is mainly localized in the nuclei and ER and that during HCV infection the amount of NOX4 in the nucleus increases , which seems to be one of the mechanisms underlying HCV pathogenesis. Therefore, it is also possible to speculate that nuclear NOX4 may increase during the acute phase of HCV infection in our experimental system, thus promoting the DNA damage and apoptosis of infected cells. Apoptotic death might favor virus spread throughout the cell culture. Further studies are in progress to deepen this aspect.
It is important to note, however, that NOXs are not the only source of ROS production in HCV-infected cells . In fact, some viral proteins, i.e., core, NS3/NS4A, and NS5A, have been shown to increase ROS levels [7, 9, 52–54] through direct or indirect interaction with mitochondria. Therefore, we cannot rule out that ROS increase in HCV-infected cells might be in part produced by mitochondrial compartment, other than NOXs.
Because of high chemical reactivity of ROS, cells possess antioxidant defense mechanisms for maintaining redox homeostasis , whose principal component is GSH, the main abundant intracellular antioxidant. It plays a crucial role in sustaining redox balance, and the ratio of GSH to GSSG is considered as a good indicator of the redox environment. To date, there is a great debate on the induction and modulation of oxidative stress by HCV and its relationship with acute or chronic phase of infection.
Hepatocytes are the major source of GSH in the body, and the GSH antioxidant system plays an important role against oxidative stress in these cells . Interestingly, reduced GSH levels were found in the serum and liver of chronically HCV-infected patients [28, 57]. Here, we found that intracellular GSH levels were significantly decreased in infected cells during the acute phase, while those of GSSG were increased, and, consequently, the ratio GSH/GSSG shifted toward GSSG, thus reflecting an impaired antioxidant potential. The oxidized environment seems to be necessary for HCV to replicate as demonstrated by viral titer peak in the acute phase. These data are in line with different in vitro studies on viruses responsible for acute infection, demonstrating the role of virus-induced oxidative stress in promoting viral replication [48, 50, 58–60]. On the contrary, during the chronic phase, reducing redox environment was restored by increased GSH content in infected cells that might be useful for the establishment of viral persistence. Indeed, treatment of persistently HCV-infected cells with the prooxidant drug auranofin caused the reactivation of HCV replication. The mechanisms through which HCV manipulates redox environment to its advantage are not fully clarified yet.
It is known that GSH de novo synthesis is driven by Nrf2 (nuclear factor erythroid 2-related factor), one of the major cellular defense mechanisms against oxidative stress and a master regulator of different cytoprotective genes including those involved in the antioxidant GSH pathway . It has been recently demonstrated that higher expression of nuclear Nrf2 contributes to persistent HCV infection and that knockdown of Nrf2 suppresses its persistent infection . The authors suggest that the nuclear translocation of p-Nrf2 might play an important role in the expression of the genes which contribute to regulate apoptosis and HCV persistence [25, 26, 30, 62]. Accordingly, we found higher mRNA levels of GCL and GS enzymes during the recovery period; at the same time, Nrf2 protein content was highly expressed during the chronic phase. On the basis of these evidences, we suggest that the high GSH levels registered in chronically infected cells compared to those measured during the acute phase of infection might be partly related to the activation of Nrf2 pathway.
There is a great debate regarding the supplementation of antioxidants in combination with antiviral drugs. In fact several clinical trials reported that antioxidant therapy decreases viral load and ameliorates hepatic damage . However, other studies reported that supplementation with vitamin C, E, and selenium increased the antioxidant status but had no effects on viral load or oxidative markers . All these conflicting results highlight the “dark side” of some antioxidants. Therefore, on the basis of our evidences and on the literature available, we suggest to carefully consider the use of antioxidants in chronically HCV-infected patients, since, although they could limit liver tissue injury, they would contribute to establish virus persistence that, in turn, can contribute to the development of hepatocellular carcinoma.
The lack of HCV vaccine and the emergence of viral strains resistant to antiviral therapy underline our limits in the current weapons used to fight the infection. In the recent years, new drugs acting specifically on HCV viral proteins (DAA) have been developed among which are the inhibitors of protease (telaprevir, boceprevir, and simeprevir) and the last approved RNA polymerase inhibitor, sofosbuvir . Since the emergence of drug-resistant HCV variants has been recently described , there is an urgent need to identify novel targets for the design of new effective therapeutic strategies. In this context, targeting of redox-sensitive host-cells pathways essential for viral replication and/or persistence may represent a promising option for contrasting HCV infection.
In conclusion, we demonstrate that the acute phase of HCV infection is characterized by a marked oxidative stress that, similarly to other viruses, is useful for viral replication. On the contrary, the restoration of reducing redox conditions that characterize the chronic phase of infection might play a key role in decreasing viral replication and apoptotic death. Overall, our data indicate that redox sensitive pathways control the different phases of HCV infection and suggest a particular wariness in the supplementation of exogenous antioxidants in chronically HCV-infected patients for their potential role in favoring viral persistence.
The data used to support the findings of this study are available from the corresponding author upon request.
Conflicts of Interest
The authors declare that there is no conflict of interests.
S. Anticoli and D. Amatore equally contributed to the execution of the experiments and drafted the paper; A.Ruggieri and L. Nencioni conceived the idea, designed the study, participated to the analysis and interpretation of data, and supervised the manuscript; M. De Angelis was in charge of western blotting experiments; P. Matarrese was in charge of the flow cytometry experimental analysis and interpretation of the resulting data; AT Palamara was the overall supervisor.
The authors are grateful to Prof. C. Rice for kindly providing the Jc1 infectious clone, FL-J6/JFH1-5C19RLuc 2Ubi plasmid. The research was supported in part by a research grant to SA provided by Prof. AT Palamara. The research was further supported in part by the Italian Ministry of Education, University and Research - MIUR PRIN (ATP), Ateneo (LN, ATP) grants, Istituto Superiore di Sanità intramural funds (AR), Italian Association for Cancer Research (N.18526 2016 to PM), Arcobaleno Onlus (PM), and the Italian INAIL-BRIC (ID50 2016 to AR).
- WHO, “Global hepatitis report,” 2017, https://www.who.int/hepatitis/publications/global-hepatitis-report2017/en/.
- R. H. Westbrook and G. Dusheiko, “Natural history of hepatitis C,” Journal of Hepatology, vol. 61, no. 1, pp. S58–S68, 2014.
- S. Clément, S. Pascarella, and F. Negro, “Hepatitis C Virus infection: molecular pathways to steatosis, insulin resistance and oxidative stress,” Viruses, vol. 1, no. 2, pp. 126–143, 2009.
- K. Tanikawa and T. Torimura, “Studies on oxidative stress in liver diseases: important future trends in liver research,” Medical Molecular Morphology, vol. 39, no. 1, pp. 22–27, 2006.
- K. de Andrade, F. Moura, J. dos Santos, O. de Araújo, J. de Farias Santos, and M. Goulart, “Oxidative stress and inflammation in hepatic diseases: therapeutic possibilities of N-acetylcysteine,” International Journal of Molecular Sciences, vol. 16, no. 12, pp. 30269–30308, 2015.
- C. Bureau, J. Bernad, N. Chaouche et al., “Nonstructural 3 protein of hepatitis C virus triggers an oxidative burst in human monocytes via activation of NADPH oxidase,” The Journal of Biological Chemistry, vol. 276, no. 25, pp. 23077–23083, 2001.
- G. Gong, G. Waris, R. Tanveer, and A. Siddiqui, “Human hepatitis C virus NS5A protein alters intracellular calcium levels, induces oxidative stress, and activates STAT-3 and NF-κB,” Proceedings of the National Academy of Sciences of the United States of America, vol. 98, no. 17, pp. 9599–9604, 2001.
- N. Fu, H. Yao, Y. Nan, and L. Qiao, “Role of oxidative stress in hepatitis C virus induced hepatocellular carcinoma,” Current Cancer Drug Targets, vol. 17, no. 6, pp. 498–504, 2017.
- M. Okuda, K. Li, M. R. Beard et al., “Mitochondrial injury, oxidative stress, and antioxidant gene expression are induced by hepatitis C virus core protein,” Gastroenterology, vol. 122, no. 2, pp. 366–375, 2002.
- G. Waris, J. Turkson, T. Hassanein, and A. Siddiqui, “Hepatitis C virus (HCV) constitutively activates STAT-3 via oxidative stress: role of STAT-3 in HCV replication,” Journal of Virology, vol. 79, no. 3, pp. 1569–1580, 2005.
- S. Pal, S. J. Polyak, N. Bano et al., “Hepatitis C virus induces oxidative stress, DNA damage and modulates the DNA repair enzyme NEIL1,” Journal of Gastroenterology and Hepatology, vol. 25, no. 3, pp. 627–634, 2010.
- S. Blackham, A. Baillie, F. al-Hababi et al., “Gene expression profiling indicates the roles of host oxidative stress, apoptosis, lipid metabolism, and intracellular transport genes in the replication of hepatitis C virus,” Journal of Virology, vol. 84, no. 10, pp. 5404–5414, 2010.
- R. Medvedev, D. Ploen, and E. Hildt, “HCV and oxidative stress: implications for HCV life cycle and HCV-associated pathogenesis,” Oxidative Medicine and Cellular Longevity, vol. 2016, Article ID 9012580, 13 pages, 2016.
- A. V. Ivanov, V. T. Valuev-Elliston, D. A. Tyurina et al., “Oxidative stress, a trigger of hepatitis C and B virus-induced liver carcinogenesis,” Oncotarget, vol. 8, no. 3, pp. 3895–3932, 2017.
- A. Ivanov, O. Smirnova, I. Petrushanko et al., “HCV core protein uses multiple mechanisms to induce oxidative stress in human hepatoma Huh7 cells,” Viruses, vol. 7, no. 6, pp. 2745–2770, 2015.
- O. A. Smirnova, O. N. Ivanova, B. Bartosch et al., “Hepatitis C virus NS5A protein triggers oxidative stress by inducing NADPH oxidases 1 and 4 and cytochrome P450 2E1,” Oxidative Medicine and Cellular Longevity, vol. 2016, Article ID 8341937, 10 pages, 2016.
- A. V. Ivanov, O. A. Smirnova, O. N. Ivanova, O. V. Masalova, S. N. Kochetkov, and M. G. Isaguliants, “Hepatitis C virus proteins activate NRF2/ARE pathway by distinct ROS-dependent and independent mechanisms in HUH7 cells,” PLoS One, vol. 6, no. 9, article e24957, 2011.
- C. X. C. Santos, L. Y. Tanaka, J. Wosniak Jr, and F. R. M. Laurindo, “Mechanisms and implications of reactive oxygen species generation during the unfolded protein response: roles of endoplasmic reticulum oxidoreductases, mitochondrial electron transport, and NADPH oxidase,” Antioxidants & Redox Signaling, vol. 11, no. 10, pp. 2409–2427, 2009.
- N. S. R. de Mochel, S. Seronello, S. H. Wang et al., “Hepatocyte NAD(P)H oxidases as an endogenous source of reactive oxygen species during hepatitis C virus infection,” Hepatology, vol. 52, no. 1, pp. 47–59, 2010.
- M. Y. Abdalla, I. M. Ahmad, D. R. Spitz, W. N. Schmidt, and B. E. Britigan, “Hepatitis C virus-core and non structural proteins lead to different effects on cellular antioxidant defenses,” Journal of Medical Virology, vol. 76, no. 4, pp. 489–497, 2005.
- C. Brault, P. Lévy, S. Duponchel et al., “Glutathione peroxidase 4 is reversibly induced by HCV to control lipid peroxidation and to increase virion infectivity,” Gut, vol. 65, no. 1, pp. 144–154, 2016.
- A. Kasprzak and A. Adamek, “Role of hepatitis C virus proteins (C, NS3, NS5A) in hepatic oncogenesis,” Hepatology Research, vol. 38, no. 1, pp. 1–26, 2008.
- D. L. Diamond, A. J. Syder, J. M. Jacobs et al., “Temporal proteome and lipidome profiles reveal hepatitis C virus-associated reprogramming of hepatocellular metabolism and bioenergetics,” PLoS Pathogens, vol. 6, no. 1, article e1000719, 2010.
- H. J. Forman and D. A. Dickinson, “Oxidative signaling and glutathione synthesis,” BioFactors, vol. 17, no. 1-4, pp. 1–12, 2003.
- D. Burdette, M. Olivarez, and G. Waris, “Activation of transcription factor Nrf2 by hepatitis C virus induces the cell-survival pathway,” The Journal of General Virology, vol. 91, no. 3, pp. 681–690, 2010.
- M. Carvajal-Yepes, K. Himmelsbach, S. Schaedler et al., “Hepatitis C virus impairs the induction of cytoprotective Nrf2 target genes by delocalization of small Maf proteins,” The Journal of Biological Chemistry, vol. 286, no. 11, pp. 8941–8951, 2011.
- B. Roe, E. Kensicki, R. Mohney, and W. W. Hall, “Metabolomic profile of hepatitis C virus-infected hepatocytes,” PLoS One, vol. 6, no. 8, article e23641, 2011.
- M. S. Farias, P. Budni, C. M. Ribeiro et al., “Antioxidant supplementation attenuates oxidative stress in chronic hepatitis C patients,” Gastroenterología y Hepatología, vol. 35, no. 6, pp. 386–394, 2012.
- M. H. Khadem Ansari, M. D. Omrani, and F. Kheradmand, “Oxidative stress response in patients infected by diverse hepatitis C virus genotypes,” Hepatitis Monthly, vol. 15, no. 2, article e22069, 2015.
- R. Medvedev, D. Ploen, C. Spengler et al., “HCV-induced oxidative stress by inhibition of Nrf2 triggers autophagy and favors release of viral particles,” Free Radical Biology & Medicine, vol. 110, pp. 300–315, 2017.
- K. J. Blight, J. A. McKeating, and C. M. Rice, “Highly permissive cell lines for subgenomic and genomic hepatitis C virus RNA replication,” Journal of Virology, vol. 76, no. 24, pp. 13001–13014, 2002.
- B. D. Lindenbach, M. J. Evans, A. J. Syder et al., “Complete replication of hepatitis C virus in cell culture,” Science, vol. 309, no. 5734, pp. 623–626, 2005.
- L. J. Reed and H. Muench, “A simple method of estimating fifty per cent endpoints,” American Journal of Epidemiology, vol. 27, no. 3, pp. 493–497, 1938.
- J. Choi, N. L. B. Corder, B. Koduru, and Y. Wang, “Oxidative stress and hepatic Nox proteins in chronic hepatitis C and hepatocellular carcinoma,” Free Radical Biology & Medicine, vol. 72, pp. 267–284, 2014.
- A. Ruggieri, S. Anticoli, L. Nencioni, R. Sgarbanti, E. Garaci, and A. Palamara, “Interplay between hepatitis C virus and redox cell signaling,” International Journal of Molecular Sciences, vol. 14, no. 3, pp. 4705–4721, 2013.
- H. E. Boudreau, S. U. Emerson, A. Korzeniowska, M. A. Jendrysik, and T. L. Leto, “Hepatitis C virus (HCV) proteins induce NADPH oxidase 4 expression in a transforming growth factor β-dependent manner: a new contributor to HCV-induced oxidative stress,” Journal of Virology, vol. 83, no. 24, pp. 12934–12946, 2009.
- A. Meister and M. E. Anderson, “Glutathione,” Annual Review of Biochemistry, vol. 52, no. 1, pp. 711–760, 1983.
- A. Meister and S. S. Tate, “Glutathione and related γ-glutamyl compounds: biosynthesis and utilization,” Annual Review of Biochemistry, vol. 45, no. 1, pp. 559–604, 1976.
- V. Gandin and A. Fernandes, “Metal- and semimetal-containing inhibitors of thioredoxin reductase as anticancer agents,” Molecules, vol. 20, no. 7, pp. 12732–12756, 2015.
- M. G. Lewis, S. DaFonseca, N. Chomont et al., “Gold drug auranofin restricts the viral reservoir in the monkey AIDS model and induces containment of viral load following ART suspension,” AIDS, vol. 25, no. 11, pp. 1347–1356, 2011.
- J. M. Madeira, S. M. Schindler, and A. Klegeris, “A new look at auranofin, dextromethorphan and rosiglitazone for reduction of glia-mediated inflammation in neurodegenerative diseases,” Neural Regeneration Research, vol. 10, no. 3, pp. 391–393, 2015.
- K. D. Tardif, G. Waris, and A. Siddiqui, “Hepatitis C virus, ER stress, and oxidative stress,” Trends in Microbiology, vol. 13, no. 4, pp. 159–163, 2005.
- K. Moriya, K. Nakagawa, T. Santa et al., “Oxidative stress in the absence of inflammation in a mouse model for hepatitis C virus-associated hepatocarcinogenesis,” Cancer Research, vol. 61, no. 11, pp. 4365–4370, 2001.
- J. Zhong, P. Gastaminza, J. Chung et al., “Persistent hepatitis C virus infection in vitro: coevolution of virus and host,” Journal of Virology, vol. 80, no. 22, pp. 11082–11093, 2006.
- K. Bedard and K. H. Krause, “The NOX family of ROS-generating NADPH oxidases: physiology and pathophysiology,” Physiological Reviews, vol. 87, no. 1, pp. 245–313, 2007.
- T. Luangmonkong, S. Suriguga, H. A. M. Mutsaers, G. M. M. Groothuis, P. Olinga, and M. Boersema, “Targeting oxidative stress for the treatment of liver fibrosis,” Reviews of Physiology, Biochemistry and Pharmacology, vol. 175, pp. 71–102, 2018.
- S. Liang, T. Kisseleva, and D. A. Brenner, “The role of NADPH oxidases (NOXs) in liver fibrosis and the activation of myofibroblasts,” Frontiers in Physiology, vol. 7, p. 17, 2016.
- D. Amatore, R. Sgarbanti, K. Aquilano et al., “Influenza virus replication in lung epithelial cells depends on redox-sensitive pathways activated by NOX4-derived ROS,” Cellular Microbiology, vol. 17, no. 1, pp. 131–145, 2015.
- R. Vlahos, J. Stambas, S. Bozinovski, B. R. S. Broughton, G. R. Drummond, and S. Selemidis, “Inhibition of Nox2 oxidase activity ameliorates influenza A virus-induced lung inflammation,” PLoS Pathogens, vol. 7, no. 2, article e1001271, 2011.
- I. Celestino, P. Checconi, D. Amatore et al., “Differential redox state contributes to sex disparities in the response to influenza virus infection in male and female mice,” Frontiers in Immunology, vol. 9, p. 1747, 2018.
- T. Wang and S. A. Weinman, “Interactions between hepatitis C virus and mitochondria: impact on pathogenesis and innate immunity,” Current Pathobiology Reports, vol. 1, no. 3, pp. 179–187, 2013.
- M. V. García-Mediavilla, S. Sánchez-Campos, P. González-Pérez et al., “Differential contribution of hepatitis C virus NS5A and core proteins to the induction of oxidative and nitrosative stress in human hepatocyte-derived cells,” Journal of Hepatology, vol. 43, no. 4, pp. 606–613, 2005.
- K. Machida, K. T.-H. Cheng, C.-K. Lai, K.-S. Jeng, V. M.-H. Sung, and M. M. C. Lai, “Hepatitis C virus triggers mitochondrial permeability transition with production of reactive oxygen species, leading to DNA damage and STAT3 activation,” Journal of Virology, vol. 80, no. 14, pp. 7199–7207, 2006.
- L. C. Robinson and J. S. Marchant, “Enhanced Ca2+ leak from ER Ca2+ stores induced by hepatitis C NS5A protein,” Biochemical and Biophysical Research Communications, vol. 368, no. 3, pp. 593–599, 2008.
- M. Valko, D. Leibfritz, J. Moncol, M. T. D. Cronin, M. Mazur, and J. Telser, “Free radicals and antioxidants in normal physiological functions and human disease,” The International Journal of Biochemistry & Cell Biology, vol. 39, no. 1, pp. 44–84, 2007.
- M. Marí, A. Morales, A. Colell, C. García-Ruiz, and J. C. Fernández-Checa, “Mitochondrial glutathione, a key survival antioxidant,” Antioxidants & Redox Signaling, vol. 11, no. 11, pp. 2685–2700, 2009.
- C. Espinosa-Diez, V. Miguel, D. Mennerich et al., “Antioxidant responses and cellular adjustments to oxidative stress,” Redox Biology, vol. 6, pp. 183–197, 2015.
- L. Nencioni, R. Sgarbanti, D. Amatore et al., “Intracellular redox signaling as therapeutic target for novel antiviral strategy,” Current Pharmaceutical Design, vol. 17, no. 35, pp. 3898–3904, 2011.
- R. C. Gullberg, J. Jordan Steel, S. L. Moon, E. Soltani, and B. J. Geiss, “Oxidative stress influences positive strand RNA virus genome synthesis and capping,” Virology, vol. 475, pp. 219–229, 2015.
- Y.‐. H. Wu, C.-P. Tseng, M.-L. Cheng, H.-Y. Ho, S.-R. Shih, and D. T.-Y. Chiu, “Glucose-6-phosphate dehydrogenase deficiency enhances human coronavirus 229E infection,” The Journal of Infectious Diseases, vol. 197, no. 6, pp. 812–816, 2008.
- S. Vomund, A. Schäfer, M. Parnham, B. Brüne, and A. von Knethen, “Nrf2, the master regulator of anti-oxidative responses,” International Journal of Molecular Sciences, vol. 18, no. 12, p. 2772, 2017.
- K. Sugiyama, H. Ebinuma, N. Nakamoto et al., “Prominent steatosis with hypermetabolism of the cell line permissive for years of infection with hepatitis C virus,” PLoS One, vol. 9, no. 4, article e94460, 2014.
- S. A. Lozano-Sepulveda, O. L. Bryan-Marrugo, C. Cordova-Fletes, M. C. Gutierrez-Ruiz, and A. M. Rivas-Estilla, “Oxidative stress modulation in hepatitis C virus infected cells,” World Journal of Hepatology, vol. 7, no. 29, pp. 2880–2889, 2015.
- K. Groenbaek, H. Friis, M. Hansen, H. Ring-Larsen, and H. B. Krarup, “The effect of antioxidant supplementation on hepatitis C viral load, transaminases and oxidative status: a randomized trial among chronic hepatitis C virus-infected patients,” European Journal of Gastroenterology & Hepatology, vol. 18, no. 9, pp. 985–989, 2006.
- J. Vermehren, J. S. Park, I. M. Jacobson, and S. Zeuzem, “Challenges and perspectives of direct antivirals for the treatment of hepatitis C virus infection,” Journal of Hepatology, vol. 69, no. 5, pp. 1178–1187, 2018.
- S. Bagaglio, C. Uberti-Foppa, and G. Morsica, “Resistance mechanisms in hepatitis C virus: implications for direct-acting antiviral use,” Drugs, vol. 77, no. 10, pp. 1043–1055, 2017.
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