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Expression of Biliverdin Reductase A in Peripheral Blood Leukocytes Is Associated with Treatment Response in HCV-Infected Patients

  • Iva Subhanova ,

    Affiliation Institute of Medical Biochemistry and Laboratory Diagnostics, General University Hospital and 1st Faculty of Medicine, Charles University in Prague, Prague, Czech Republic

  • Lucie Muchova,

    Affiliation Institute of Medical Biochemistry and Laboratory Diagnostics, General University Hospital and 1st Faculty of Medicine, Charles University in Prague, Prague, Czech Republic

  • Martin Lenicek,

    Affiliation Institute of Medical Biochemistry and Laboratory Diagnostics, General University Hospital and 1st Faculty of Medicine, Charles University in Prague, Prague, Czech Republic

  • Hendrik J. Vreman,

    Affiliation Department of Pediatrics, Stanford University School of Medicine, Stanford, California, United States of America

  • Ondrej Luksan,

    Affiliation Centre of Experimental Medicine, Institute for Clinical and Experimental Medicine, Prague, Czech Republic

  • Kristyna Kubickova,

    Affiliation Department of Internal Medicine, 1st Faculty of Medicine, Charles University in Prague, Prague, Czech Republic

  • Miluse Kreidlova,

    Affiliation Institute of Medical Biochemistry and Laboratory Diagnostics, General University Hospital and 1st Faculty of Medicine, Charles University in Prague, Prague, Czech Republic

  • Tomas Zima,

    Affiliation Institute of Medical Biochemistry and Laboratory Diagnostics, General University Hospital and 1st Faculty of Medicine, Charles University in Prague, Prague, Czech Republic

  • Libor Vitek ,

    Contributed equally to this work with: Libor Vitek, Petr Urbanek

    Affiliations Institute of Medical Biochemistry and Laboratory Diagnostics, General University Hospital and 1st Faculty of Medicine, Charles University in Prague, Prague, Czech Republic, 4th Department of Internal Medicine, 1st Faculty of Medicine, Charles University in Prague, Prague, Czech Republic

  • Petr Urbanek

    Contributed equally to this work with: Libor Vitek, Petr Urbanek

    Affiliation Department of Internal Medicine, 1st Faculty of Medicine, Charles University in Prague, Prague, Czech Republic

Expression of Biliverdin Reductase A in Peripheral Blood Leukocytes Is Associated with Treatment Response in HCV-Infected Patients

  • Iva Subhanova, 
  • Lucie Muchova, 
  • Martin Lenicek, 
  • Hendrik J. Vreman, 
  • Ondrej Luksan, 
  • Kristyna Kubickova, 
  • Miluse Kreidlova, 
  • Tomas Zima, 
  • Libor Vitek, 
  • Petr Urbanek


Background and Aims

Hepatitis C virus (HCV) infection is associated with systemic oxidative stress. Since the heme catabolic pathway plays an important role in antioxidant protection, we attempted to assess the gene expression of key enzymes of heme catabolism, heme oxygenase 1 (HMOX1), heme oxygenase 2 (HMOX2), and biliverdin reductase A (BLVRA) in the liver and peripheral blood leukocytes (PBL) of patients chronically infected with HCV.


Gene expressions (HMOX1, HMOX2, BLVRA) and HCV RNA were analyzed in PBL of HCV treatment naïve patients (n = 58) and controls (n = 55), with a subset of HCV patients having data on hepatic gene expression (n = 35). Based upon the therapeutic outcome, HCV patients were classified as either responders (n = 38) or treatment-failure patients (n = 20). Blood samples in HCV patients were collected at day 0, and week 12, 24, 36, and 48 after the initiation of standard antiviral therapy.


Compared to the controls, substantially increased BLVRA expression was detected in PBL (p<0.001) of therapeutically naïve HCV patients. mRNA levels of BLVRA in PBL closely correlated with those in liver tissue (r2 = 0.347,p = 0.03). A marked difference in BLVRA expression in PBL between the sustained responders and patients with treatment failure was detected at week 0 and during the follow-up (p<0.001). Multivariate analysis revealed that BLVRA basal expression in PBL was an independent predictor for sustained virological response (OR 15; 95% CI 1.05–214.2; P = 0.046). HMOX1/2 expression did not have any effect on the treatment outcome.


Our results suggest that patients with chronic HCV infection significantly upregulate BLVRA expression in PBL. The lack of BLVRA overexpression is associated with non-responsiveness to standard antiviral therapy; whereas, HMOX1/2 does not seem to have any predictive potential.


Hepatitis C virus (HCV) infection represents one of the leading causes of chronic hepatitis worldwide, resulting in progression into fibrosis, cirrhosis and hepatocellular carcinoma in a significant number of HCV-infected patients [1]. The HCV prevalence is estimated to be 3% worldwide [2] and 0.2–0.5% in the Czech Republic with predominance of genotype 1 (79.3%) and 3 (19.7%) [3], [4].

Although HCV is mainly hepatotropic, there is also evidence that it can replicate in the peripheral blood mononuclear cells (PBMC) of patients with chronic HCV infection [5].

Oxidative damage has been hypothesized to play a role in HCV-induced liver disease, with reactive oxygen and nitrogen species (RONS) generated from HCV-infected hepatocytes, and infiltrating the immune cells [6], [7]. HCV might not only increase RONS production, but also downregulate expression of certain antioxidant genes, including heme oxygenase (HMOX) [8]. HMOX catalyzes the degradation of the pro-oxidative heme to biliverdin, carbon monoxide (CO), and iron (Figure 1). Biliverdin is then subsequently reduced to bilirubin by biliverdin reductase (BLVR). Biliverdin, bilirubin, and CO exert numerous biological functions, including anti-oxidative and anti-inflammatory effects, as well as the modulation of cell proliferation and apoptosis [9], [10], [11]. Two HMOX isoforms have evolved, which include HMOX1 (OMIM*141250), an inducible isoenzyme, and HMOX2 (OMIM*141251), a constitutive isoform. Both catalyze the same reaction, but are differentially regulated, and play different roles in protecting tissues against oxidative injuries [12]. An accumulating body of evidence suggests that HMOX1 overexpression contributes to cellular response against oxidative stress [13], and might have strong anti-fibrotic, as well as an anti-apoptotic potential within the liver tissue [14], [15]. HMOX1 induction in vitro has recently been shown to decrease HCV replication [16]. On the other hand, reduced HMOX1 expression has been reported in the liver tissue of patients with chronic hepatitis C [8]; although under in vitro conditions hepatic HMOX1 overexpression in the presence of HCV proteins has been reported by other authors [17].

Figure 1. Heme catabolic pathway.

Heme oxygenase, the rate limiting enzyme in the heme catabolic pathway, catalyzes oxidative degradation of heme to form equimolar amounts of bioactive products carbon monoxide, iron and biliverdin, which is subsequently reduced to bilirubin by biliverdin reductase.

BLVR, the other enzyme involved in the heme catabolic pathway, is also implicated in the oxidative stress response [18]. Apart from its antioxidative effects, a cytoprotective action independent of heme degradation has been reported [19], [20]. In fact, BLVR has been demonstrated to affect cell signaling pathways by regulating stress-responsive genes, including both HMOX1 [21], [22], and HMOX2 [23]. Two isoforms of human BLVR, BLVRA (OMIM*109750) and BLVRB (OMIM*600941), products of different genes, have been described [24]. BLVRA, the major form of BLVR in the human adult liver, is subject to regulation by tumor necrosis factor-α, as well as by oxidative stress or hypoxia [25]. Importantly, biliverdin has been shown to inhibit HCV replication [26]. Lehmann et al. [26] recently demonstrated that biliverdin interferes with HCV replication-mediated oxidative stress by inducing the expression of antiviral interferons. Huang et al. [27] reported an association between sustained virological response (SVR) and expression of BLVRB, the embryonic form of BLVR in PBMC during the first weeks of antiviral therapy. However, no data are available on BLVRA expression in the liver, or PBL in chronic HCV infection.

Therefore, the present study was conducted to evaluate the possible role of HCV infection on HMOX1/HMOX2/BLVRA gene expression in the liver and PBL, as well as whether these genes may influence or predict the treatment response.

Patients and Methods


The study was performed on 58 consecutive therapeutically naïve patients with chronic HCV infection. The patients were recruited between 2007–2011 at the Hepatology Center in the Central Military Hospital in Prague, Czech Republic. Patients with positivity of anti-HCV antibodies, and detectable HCV RNA in serum for at least 6 months, were included in the study. Detailed description of patients enrolled is given in Table 1.

The patients received standard antiviral therapy (pegylated interferon alpha in combination with ribavirin (PEG-IFN-alpha/RBV)) according to EASL and AASLD practice guidelines [28]. The treatment regimens were: 1) PEG-IFN alpha 2a (Pegasys; Roche, Basel, Switzerland): 180 µg once weekly+RBV (Copegus; Roche, Basel, Switzerland ) 1000–1200 mg daily, according to body weight (1000 mg ≤75 kg, 1200 mg >75 kg); and 2) PEG-IFN alpha-2b (PegIntron; Schering-Plough, Kenilworth, NJ, USA): 1.5 µg/kg body weight once weekly+RBV (Rebetol; Schering-Plough, Kenilworth, NJ, USA): 1000–1200 mg daily, according to body weight (1000 mg ≤75 kg, 1200 mg >75 kg).

The total duration of the antiviral therapy was defined by the type of antiviral response within the first 12–24 weeks of therapy. Patients with HCV RNA decrease <2 log from baseline level at week 12 were classified as null responders and their antiviral therapy was terminated at week 12. Patients with HCV RNA decrease ≥2 log or with undetectable HCV RNA at week 12 were treated to week 24. If HCV RNA was detectable at week 24, patients were classified as slow responders and their therapy was terminated at week 24. Only patients with undetectable HCV RNA at week 24 were treated up to week 48.

Based on the treatment response, patients were classified into two groups. Responders were defined as patients with sustained virologic response (SVR, undetectable HCV RNA at weeks 24 after completion of antiviral therapy, n = 38). Treatment-failure patients (non-SVR, n = 20) included those who did not achieved SVR (n = 15) and patients who relapsed (n = 5).

For PBMC and PBL studies, 55 healthy volunteers (blood donors or employees of General Faculty Hospital and 1st Faculty of Medicine, Charles University in Prague) were used as control subjects. The study was registered under ID: NCT 00842250 (

The study protocol conformed to all ethical guidelines of the 1975 Declaration of Helsinki, reflected in the a priori approval by the institution’s Ethics Committee. Additionally, all subjects in this study had provided written informed consent.


Material sampling and storage.

Patients’ blood samples were collected on the day before treatment initiation (day 0, n = 58), as well as at 12 (n = 37), 24 (n = 31), 36 (n = 27) and 48 (n = 16) weeks after initiation of the standard antiviral treatment. Samples for gene expression analyses were collected into PAXgene Blood RNA Tubes (PreAnalytix, Hombrechtikon, Switzerland) and stored at −80°C. Samples for determination of total HMOX activity in PBMC were collected in BD Vacutainer Blood collection tubes with heparin (BD Diagnostics-Preanalytical Systems, Franklin Lakes, NJ, USA). PBMC were isolated through a Ficoll-density gradient within 5 hours, and stored in potassium phosphate buffer at −80°C. The blood samples for analysis of interleukin 28B (IL28B, OMIM*607402) gene polymorphism were collected in BD Vacutainer Blood collection tubes with EDTA (BD Diagnostics-Preanalytical Systems, Franklin Lakes, NJ, USA) and stored at −80°C.

All liver samples were immediately placed into RNAlater (Ambion Diagnostics, Austin, TX, USA) and stored at −80°C until total RNA isolation.


Hemin, nicotinamide adenine dinucleotide phosphate (NADPH) and sulfosalicylic acid were purchased from Sigma (St. Louis, MO, USA). Sodium dihydrogen phosphate (NaH2PO4) and disodium hydrogen phosphate (Na2HPO4) were of analytical grade, and purchased from Penta (Prague, Czech Republic).

Markers of liver injury.

Liver biopsy samples were evaluated according to the Ishak scoring system [29]. Serum markers of liver injury (ALT, AST, GGT, ALP) and bilirubin were analyzed by routine assays on an automated analyzer (Modular analyzer, Roche Diagnostics GmbH, Mannheim, Germany).

Serological analyses.

HCV RNA in sera was quantified using Roche Cobas AmpliPrep/Cobas TaqMan (detection limit of 15 IU/ml) (Roche Diagnostics GmbH, Mannheim, Germany). HCV genotypes were analysed with VERSANT HCV Genotype 2.0 Assay (LiPA) (Siemens Healthcare Diagnostics, Camberley, UK).

Genomic DNA isolation and IL28B genotyping.

Genomic DNA was extracted from EDTA coagulated peripheral blood using MagNA Pure Compact Nucleic acid isolation Kit (Roche Diagnostics GmbH, Mannheim, Germany). The human IL28B promoter polymorphism at position −3176 (rs12979860) was analysed using LightMix Kit IL28B (TIB Molbiol GmbH, Berlin, Germany).

Total RNA isolation and reverse transcription.

The liver tissue was homogenized using a MagNA Lyser System (Roche Applied Science, Mannheim, Germany), according to the manufacturer’s instructions. Total RNA from the homogenized liver tissue was isolated using RNeasy Mini (Qiagen, Dallas, TX, USA), and total RNA from PBL using a PAXgene kit (Qiagen, Dallas, TX, USA), according to the manufacturer’s instructions. DNase treatment with the RNase-free DNase (Qiagen, Dallas, TX, USA), prior to cDNA synthesis, was carried out according to the manufacturer’s instructions. The RNA integrity was checked by agarose gel electrophoresis. First-strand cDNA was synthesized from 0,2 µg of total RNA in a final volume of 20 µl using a High-Capacity cDNA kit according to the manufacturer’s instructions (Applied Biosystems, Foster City, CA, USA).

RealTime HCV RNA and gene expression quantification.

The HCV Primer sequences were based on data by Carriere et al. [30]. Other primers were designed using Primer 3 software ( Accessed 2013 Feb 1) and synthesized by Generi Biotech (Hradec Kralove, Czech Republic) (Table 2).

Table 2. Primer sequences for HCV RNA, target and internal control genes.

To determine the relative expression level of all data analysis, HPRT expression levels were measured as internal controls. The delta cycle threshold value (Δct) was calculated from the given ct value by the formula: Δct = (ct sample – ct control). The fold change was calculated as ( = 2−Δct). Two reference genes (HPRT, GAPD) were selected as the most stable among 4 constant genes (HPRT, GAPD, 18S RNA, UBC) based on the analyses of 10 PBL of HCV infected patients and controls, and 10 liver samples of HCV infected patients by using geNORM 3.5 ( Accessed 2009 Dec 15). Based upon similar expression levels as target genes, HPRT was found a more appropriate control gene, compared to GAPD.

qPCR was performed in 20 µl reaction volume, containing 4 µl of five-fold diluted cDNA template from completed RT reaction, 1× SYBR Green Master Mix (Applied Biosystems, Foster City, CA, USA), and 200 nM forward and reverse primers. All RT-PCR were set up in 96-well optical plates, and run on an ABI PRISM 7500 Sequence Detector System (Applied Biosystems, Foster City, CA, USA).

The cycling conditions included polymerase activation at 95°C for 10 min, followed with 40 cycles of 95°C for 15 s, and 60°C for 60 s. PCR products were subjected to a melting curve analysis. All samples were analyzed in triplicates. Linearized constructs for the PCR validation procedure were prepared using a TOPO TA Cloning Kit, according to the manufacturer’s instructions (Invitrogen, Carlsbad, CA, USA). PCR efficiencies for target and housekeeping cDNA were 97–105%.

HMOX activity in PBMC.

Twenty µl of PBMC sonicate (2 million cells per reaction) were incubated for 15 min at 37°C in CO-free septum-sealed vials containing 20 µl of 150 µM methemalbumin and 20 µl of 4.5 mM NADPH, as previously described [31]. Blank reaction vials contained 0.1 M phosphate buffer, pH = 7.4 in place of NADPH. The reactions were terminated by adding 5 µl of 30% (w/v) sulfosalicylic acid. The amount of CO generated by the reaction and released into the vial headspace was quantified by gas chromatography (GC) with a Reduction Gas Analyzer (Trace Analytical Laboratories, now: AMETEK Process Instrument, Newark, DE, USA). HMOX activity was calculated as pmol CO/hr/106 cells.

Statistical analysis.

The data are presented as the mean ± standard deviation (SD), or median (IQ range). Differences between the studied groups (HCV vs. controls, SVR vs. treatment-failure patients) were evaluated by an unpaired t-test, or Mann-Whitney U test. The significance of the relationship between BLVRA expression and the treatment outcome was determined by the chi-square test. Linear regression, Pearson’s correlation and multivariate logistic regression analyses were performed using SigmaStat software, version 3.01, for the statistical analysis. For multiple logistic regression analysis following clinically relevant variables were included: BLVRA expression in PBL, IL28B gene variants, HCV RNA levels, stage of liver fibrosis, gender, hemoglobin levels and platelet number. All analyses were performed with alpha set to 0.05.


Basal Expression of BLVRA in PBL of HCV Patients

BLVRA expression in PBL was markedly increased in HCV-infected patients before antiviral treatment, when compared to the control group (1.68±0.68 vs. 1.28±0.36, respectively, p<0.001). Simultaneously, baseline mRNA levels of BLVRA were significantly higher only in patients who achieved SVR, compared to the control group (1.87±0.74 vs. 1.28±0.36, respectively, p<0.001), but not in non-SVR patients (1.32±0.34 vs. 1.28±0.36 p = 0.65). The BLVRA expression in PBL of relapse patients (n = 5) before antiviral treatment was substantially reduced compared to SVR patients (1.15±0.19 vs. 1.87±0.74, p<0.001), and was also decreased, although non-significantly, when compared to non-SVR patients (n = 15) (1.15±0.19 vs. 1.32±0.34, p = 0.09). Significant differences in basal BLVRA expression were found between SVR and non-SVR patients (Table 1). When assessing possible factors responsible for treatment response, only BLVRA expression has been found to be a strong predictor (Table 3). Exclusion of BLVRA from multivariant analysis did not have any effect on predictive value of tested variables. Based on ROC analysis (Figure 2), BLVRA expression predicted the treatment response with 76% sensitivity, 70% specificity (positive predictive value = 83%, negative predictive value = 61%). Since ribavirin treatment is commonly associated with hemolysis, and bilirubin overproduction might upregulate BLVRA, we assessed the relationship between ribavirin-induced drop of hemoglobin levels and BLVRA expression (Table 4.). However, no changes in BLVRA expression were detected either in 12 or 24 weeks of antiviral therapy in hemoglobin depleted patients.

Figure 2. ROC curve of BLVRA expression in peripheral blood leukocytes of HCV infected patients.

AUC, area under the ROC curve; ROC, Receiver Operating Charasteristic.

Table 3. Multivariate logistic regression analysis of potential SVR predictors.

Expression of BLVRA in PBL in HCV Patients during Antiviral Treatment

BLVRA expression significantly increased at weeks 12 (2.57±1.61, p = 0.0004), 24 (2.57±1.17, p = 0.0002), and 36 (2.16±1.19, p = 0.03) after initiation of standard antiviral therapy when compared to the initial levels (1.68±0.68). Significant differences in BLVRA mRNA levels between SVR and non-SVR patients were found at weeks 12 and 48 after treatment initiation. Similar trends were also observed at weeks 24 and 36. These differences, however, did not reached statistical significance, most likely due to the low number of subjects (Figure.3). Interestingly, BLVRA expression in SVR patients after withdrawal of antiviral therapy (n = 10) decreased substantially compared to BLVRA expression levels at week 24 (median [IQ range] 1.38 [1.2–1.6] vs. 2.52 [1.5–2.8], p = 0.03), and reached control levels (median [IQ range] 1.38 [1.2–1.6] vs. 1.28 [1–1.5], p = 0.43).

Figure 3. BLVRA expression in peripheral blood leukocytes of responders and non-SVR patients during standard antiviral therapy.

BLVRA expression was measured the day before treatment initiation (0), and 12, 24, 36 and 48 weeks after start of the standard treatment. Data represent means and standard deviations for triplicate determinations. P-values calculated between responders and non-SVR patients. BLVRA, biliverdin reductase A; PBL, peripheral blood leukocytes; SVR = responders, NVR = non-SVR patients.

Expression and Activity of HMOX in HCV Patients

Compared to controls, the HMOX activity in PBMC of HCV-infected patients before antiviral treatment was substantially reduced (20.6±16.3 vs 36.3±18.1 pmol CO/106 cells/h, respectively, p = 0.001). Although PBL gene expression of HMOX1 did not differ between HCV-infected patients and the control group, the HMOX2 expression was slightly, but significantly, reduced in patients with HCV infection (4.30±1.13 vs 4.98±0.94, respectively, p = 0.001). While a significant correlation between PBL gene expression of HMOX1, HMOX2 mRNA and HMOX activity in PBMC was only detected in control samples (r2 = 0.210, p = 0.007; r2 = 0.113, p = 0.03), this relationship was not observed in the HCV-infected patients (r2 = 0.040, p = 0.20; r2 = 0.046, p = 0.33). Finally, no differences in either HMOX activity or HMOX expression between SVR and non-SVR patients were detected.

Correlation between BLVRA and HMOX mRNA Levels in the Liver and PBL, and HCV RNA in PBL and Liver Tissue

No significant differences in pretreatment expression of BLVRA in the liver were found between SVR (n = 18) and non-SVR patients (n = 4) (0.35±0.24 vs. 0.34±0.24 p = 0.97) most likely because of high variability of BLVRA expression in the liver compared to PBL.

BLVRA expression, but not that of HMOX1/HMOX2, in the liver and PBL of HCV-infected patients were in direct relationship (n = 13, r2 = 0.347, p = 0.03). No correlation was found between the mRNA levels of HMOX1/HMOX2/BLVRA and HCV RNA in the liver and PBL.


Because of the side effects and high costs of current antiviral therapy, it is very important to identify those markers that can discriminate among those patients who will respond to the standard treatment. The precise molecular mechanisms underlying the responsiveness to antiviral treatment among HCV-infected individuals have yet to be completely identified.

Enzymes of the heme catabolic pathway seem to belong to such promising markers. In fact, Zhu and coworkers [32] recently provided a plausible mechanism for the antiviral activity of HMOX1, demonstrating that the direct product of its activity, biliverdin, potently inhibits viral replication at biologically relevant concentrations in human hepatoma Huh-7.5 cells replicating HCV RNA, most likely via inhibition of HCV NS3/4A protease. In the current study, we prospectively investigated HMOX activity, as well as HMOX1 expression in HCV-infected patients. Surprisingly, no difference in mRNA expression of HMOX1 in PBL was found between therapeutically naïve HCV patients and controls, although the total HMOX activity in PBMC was significantly decreased in HCV patients before treatment, compared to the control group.

Furthermore, a correlation between the expression of HMOX1, HMOX2, and total HMOX activity was only detected in the control samples; not in the HCV-infected patients. In fact, interference of HCV with HMOX1 induction [33], reduced hepatic expression of HMOX1 both in vitro and in vivo in HCV infection [8]; additionally, induced hepatic HMOX1 expression in vitro were reported [17]. We hypothesized that HMOX and BLVRA gene expression in PBL can reflect their expression in the liver. In our study, due to unavailability of liver specimens of control subjects, correlation between the liver and PBL could be analyzed only in HCV patients. No association of HMOX1/HMOX2 expression was found between the liver and PBL, and HMOX1/HMOX2/BLVRA and HCV RNA in the liver and PBL. On the other hand, expression of BLVRA in the liver tissue correlated with expression of BLVRA in PBL. The expression of BLVRA in PBL was higher in HCV-infected patients before antiviral therapy, compared to the control group; and subsequently increased 12, 24, and 36 weeks after initiation of standard antiviral therapy, when compared to initial levels. Most importantly, BLVRA expression in PBL was found to be strongly associated with response to the antiviral treatment. Recent genome-wide association studies identified strong evidence IL28B gene variation (rs12979860) with SVR rates in patients chronically infected with genotype 1 HCV [34], [35], [36]. Although not statistically significant, a similar trend was observed in our cohort of patients for all genotypes (p = 0.11) as well as for genotype 1 (p = 0.16). The prevalence of CC vs non CC genotypes in our group of patients corresponds to prevalence rates of chronically infected HCV patients in the Czech Republic reported recently [37]. However, it should be noted that the lack of association with other clinically important variables tested in our regression model including IL28B gene variation might be due to small sample size effect. Furthermore, there was a clear trend for association of upregulated baseline BLVRA expression in PBL of patients with favorable CC genotype as compared to both non CC (p = 0.059) and TT IL28B (p = 0.058) patients.

Induced BLVRA gene transcription in PBMC of uninfected chimpanzees in response to INF-α [38] and in INF-α treated PBMC [39] were previously reported. In accord with this data, BLVRA overexpression in our HCV-infected patients prior to and during antiviral treatment seems to be due to BVLRA upregulation by INF-α. Moreover, our results showing an association of BLVRA in PBL with the treatment outcome are in agreement with substantially greater global induction of IFN-stimulated genes observed in the PBMC of treatment responders [40].

This data is in accord with our observation indicating that 1) SVR patients have increased BLVRA expression prior initiation of therapy (likely due to endogenous interferon induced by HCV infection); 2) both SVR and non-SVR patients have increased BLVRA expression during antiviral therapy (likely due to exogenous interferon administered therapeutically); 3) SVR patients after withdrawal of antiviral therapy have decreased expression of BLVRA to control values (likely due to decreased production of endogenous interferon, since HCV, as the major stimulus, is absent). It is also important to note, that BLVRA expression during HCV infection and antiviral therapy is independent of ribavirin-induced hemolysis. However, our data does not provide conclusive evidence whether BLVRA expression is involved actively in driving the treatment response, or is just a surrogate marker for treatment responsiveness.

In conclusion, our pilot results demonstrate that patients with chronic HCV infection significantly upregulate BLVRA expression in PBL, closely correlating with those in liver tissue. In addition, basal BLVRA expression in PBL is strongly associated with response to treatment. Finally, the lack of BLVRA overexpression is associated with non-responsiveness to standard antiviral therapy. Nevertheless, larger prospective studies are needed to confirm our data.

Author Contributions

Clinical data collection: KK PU. Revised the manuscript for important intellectual content: LM ML HJV TZ PU. Conceived and designed the experiments: IS LM ML TZ LV PU. Performed the experiments: IS OL MK. Analyzed the data: IS ML LV. Contributed reagents/materials/analysis tools: PU HJV. Wrote the paper: IS LV.


  1. 1. Seeff LB (1997) Natural history of hepatitis C. Hepatology. 26: 21S–28S.
  2. 2. World Health Organization: Hepatitis C. World Health Organization Fact sheet 164 (Revised June 2011). Available: Accessed 2012 Feb 4.
  3. 3. Nemecek V, Castkova J, Fritz P, Linhartova A, Svandova E, et al. (2003) The 2001 serological survey in the Czech Republic-viral hepatitis. Cent Eur J Public Health 11 Suppl: S54–61
  4. 4. Nemecek V, Strunecky O (2009) Genotypic heterogeneity of hepatitis C virus (HCV) from blood donors in the Czech Republic. Epidemiol Mikrobiol Imunol 58: 63–72.
  5. 5. Wang JT, Sheu JC, Lin JT, Wang TH, Chen DS (1992) Detection of replicative form of hepatitis C virus RNA in peripheral blood mononuclear cells. J Infect Dis 166: 1167–1169.
  6. 6. Peterhans E (1997) Reactive oxygen species and nitric oxide in viral diseases. Biol Trace Elem Res 56: 107–116.
  7. 7. Okuda M, Li K, Beard MR, Showalter LA, Scholle F, et al. (2002) Mitochondrial injury, oxidative stress, and antioxidant gene expression are induced by hepatitis C virus core protein. Gastroenterology 122: 366–375.
  8. 8. Abdalla MY, Britigan BE, Wen F, Icardi M, McCormick ML, et al. (2004) Down-regulation of heme oxygenase-1 by hepatitis C virus infection in vivo and by the in vitro expression of hepatitis C core protein. J Infect Dis 190: 1109–1118.
  9. 9. Sass G, Seyfried S, M PS, Yamashita K, Kaczmarek E, et al. (2004) Cooperative effect of biliverdin and carbon monoxide on survival of mice in immune-mediated liver injury. Hepatology 40: 1128–1135.
  10. 10. Verma A, Hirsch DJ, Glatt CE, Ronnett GV, Snyder SH (1993) Carbon monoxide: a putative neural messenger. Science 259: 381–384.
  11. 11. Vitek L, Schwertner HA (2007) The heme catabolic pathway and its protective effects on oxidative stress-mediated diseases. Adv Clin Chem 43: 1–57.
  12. 12. Maines MD, Panahian N (2001) The heme oxygenase system and cellular defense mechanisms. Do HO-1 and HO-2 have different functions? Adv Exp Med Biol 502: 249–272.
  13. 13. Willis D, Moore AR, Frederick R, Willoughby DA (1996) Heme oxygenase: a novel target for the modulation of the inflammatory response. Nat Med 2: 87–90.
  14. 14. Li L, Grenard P, Nhieu JT, Julien B, Mallat A, et al. (2003) Heme oxygenase-1 is an antifibrogenic protein in human hepatic myofibroblasts. Gastroenterology 125: 460–469.
  15. 15. Sass G, Soares MC, Yamashita K, Seyfried S, Zimmermann WH, et al. (2003) Heme oxygenase-1 and its reaction product, carbon monoxide, prevent inflammation-related apoptotic liver damage in mice. Hepatology 38: 909–918.
  16. 16. Zhu Z, Wilson AT, Mathahs MM, Wen F, Brown KE, et al. (2008) Heme oxygenase-1 suppresses hepatitis C virus replication and increases resistance of hepatocytes to oxidant injury. Hepatology 48: 1430–1439.
  17. 17. Ghaziani T, Shan Y, Lambrecht RW, Donohue SE, Pietschmann T, et al. (2006) HCV proteins increase expression of heme oxygenase-1 (HO-1) and decrease expression of Bach1 in human hepatoma cells. J Hepatol 45: 5–12.
  18. 18. Baranano DE, Rao M, Ferris CD, Snyder SH (2002) Biliverdin reductase: a major physiologic cytoprotectant. Proc Natl Acad Sci U S A 99: 16093–16098.
  19. 19. Miralem T, Hu Z, Torno MD, Lelli KM, Maines MD (2005) Small interference RNA-mediated gene silencing of human biliverdin reductase, but not that of heme oxygenase-1, attenuates arsenite-mediated induction of the oxygenase and increases apoptosis in 293A kidney cells. J Biol Chem 280: 17084–17092.
  20. 20. Florczyk UM, Jozkowicz A, Dulak J (2008) Biliverdin reductase: new features of an old enzyme and its potential therapeutic significance. Pharmacol Rep 60: 38–48.
  21. 21. Ahmad Z, Salim M, Maines MD (2002) Human biliverdin reductase is a leucine zipper-like DNA-binding protein and functions in transcriptional activation of heme oxygenase-1 by oxidative stress. J Biol Chem 277: 9226–9232.
  22. 22. Kravets A, Hu Z, Miralem T, Torno MD, Maines MD (2004) Biliverdin reductase, a novel regulator for induction of activating transcription factor-2 and heme oxygenase-1. J Biol Chem 279: 19916–19923.
  23. 23. Ding B, Gibbs PE, Brookes PS, Maines MD (2011) The coordinated increased expression of biliverdin reductase and heme oxygenase-2 promotes cardiomyocyte survival: a reductase-based peptide counters beta-adrenergic receptor ligand-mediated cardiac dysfunction. FASEB J 25: 301–313.
  24. 24. Yamaguchi T, Komoda Y, Nakajima H (1994) Biliverdin-IX alpha reductase and biliverdin-IX beta reductase from human liver. Purification and characterization. J Biol Chem 269: 24343–24348.
  25. 25. Maines MD (2010) Potential application of biliverdin reductase and its fragments to modulate insulin/IGF-1/MAPK/PI3-K signaling pathways in therapeutic settings. Curr Drug Targets 11: 1586–1594.
  26. 26. Lehmann E, El-Tantawy WH, Ocker M, Bartenschlager R, Lohmann V, et al. (2010) The heme oxygenase 1 product biliverdin interferes with hepatitis C virus replication by increasing antiviral interferon response. Hepatology 51: 398–404.
  27. 27. Huang C, Chen H, Cassidy W, Howell CD (2008) Peripheral blood gene expression profile associated with sustained virologic response after peginterferon plus ribavirin therapy for chronic hepatitis-C genotype 1. J Natl Med Assoc 100: 1425–1433.
  28. 28. Ghany MG, Strader DB, Thomas DL, Seeff LB (2009) Diagnosis, management, and treatment of hepatitis C: an update. Hepatology 49: 1335–1374.
  29. 29. Ishak K, Baptista A, Bianchi L, Callea F, De Groote J, et al. (1995) Histological grading and staging of chronic hepatitis. J Hepatol 22: 696–699.
  30. 30. Carriere M, Pene V, Breiman A, Conti F, Chouzenoux S, et al. (2007) A novel, sensitive, and specific RT-PCR technique for quantitation of hepatitis C virus replication. J Med Virol 79: 155–160.
  31. 31. Vreman HJ, Stevenson DK (1988) Detection of heme oxygenase activity by measurement of CO. In: Maines MD, Costa LG, Reed DJ, Sassa S, Sipes IG. Current Protocols in Toxicology. New York: John Wiley&Sons. 9.2.1–9.2.10.
  32. 32. Zhu Z, Wilson AT, Luxon BA, Brown KE, Mathahs MM, et al. (2010) Biliverdin inhibits hepatitis C virus nonstructural 3/4A protease activity: mechanism for the antiviral effects of heme oxygenase? Hepatology 52: 1897–1905.
  33. 33. Wen F, Brown KE, Britigan BE, Schmidt WN (2008) Hepatitis C core protein inhibits induction of heme oxygenase-1 and sensitizes hepatocytes to cytotoxicity. Cell Biol Toxicol 24: 175–188.
  34. 34. Ge D, Fellay J, Thompson AJ, Simon JS, Shianna KV, et al. (2009) Genetic variation in IL28B predicts hepatitis C treatment-induced viral clearance. Nature 461: 399–401.
  35. 35. Suppiah V, Moldovan M, Ahlenstiel G, Berg T, Weltman M, et al. (2009) IL28B is associated with response to chronic hepatitis C interferon-alpha and ribavirin therapy. Nat Genet 41: 1100–1104.
  36. 36. Thompson AJ, Muir AJ, Sulkowski MS, Ge D, Fellay J, et al. (2010) Interleukin-28B polymorphism improves viral kinetics and is the strongest pretreatment predictor of sustained virologic response in genotype 1 hepatitis C virus. Gastroenterology 139: 120–129.
  37. 37. Frankova S, Bartakova R, Hejda V, Urbanek P, Husova L, et al. (2012) IL28 rs 12979860 CC genotype slows progression of liver disease in HCV infected patients. Gastroenterologie a Hepatologie 66: S17.
  38. 38. Lanford RE, Guerra B, Lee H, Chavez D, Brasky KM, et al. (2006) Genomic response to interferon-alpha in chimpanzees: implications of rapid downregulation for hepatitis C kinetics. Hepatology 43: 961–972.
  39. 39. Waddell SJ, Popper SJ, Rubins KH, Griffiths MJ, Brown PO, et al. (2010) Dissecting interferon-induced transcriptional programs in human peripheral blood cells. PLoS One 5: e9753.
  40. 40. He XS, Ji X, Hale MB, Cheung R, Ahmed A, et al. (2006) Global transcriptional response to interferon is a determinant of HCV treatment outcome and is modified by race. Hepatology 44: 352–359.