Permissiveness of human hepatoma cell lines for HCV infection
© Sainz et al; licensee BioMed Central Ltd. 2011
Received: 28 November 2011
Accepted: 24 January 2012
Published: 24 January 2012
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© Sainz et al; licensee BioMed Central Ltd. 2011
Received: 28 November 2011
Accepted: 24 January 2012
Published: 24 January 2012
Although primary and established human hepatoma cell lines have been evaluated for hepatitis C virus (HCV) infection in vitro, thus far only Huh7 cells have been found to be highly permissive for infectious HCV. Since our understanding of the HCV lifecycle would benefit from the identification of additional permissive cell lines, we assembled a panel of hepatic and non-hepatic cell lines and assessed their ability to support HCV infection. Here we show infection of the human hepatoma cell lines PLC/PRF/5 and Hep3B with cell culture-derived HCV (HCVcc), albeit to lower levels than that achieved in Huh7 cells. To better understand the reduced permissiveness of PLC and Hep3B cells for HCVcc infection, we performed studies to evaluate the ability of each cell line to support specific steps of the viral lifecycle (i.e. entry, replication, egress and spread).
We found that while the early events in HCV infection (i.e. entry plus replication initiation) are cumulatively equivalent or only marginally reduced in PLC and Hep3B cells, later steps of the viral life cycle such as steady-state replication, de novo virus production and/or spread are impaired to different degrees in PLC and Hep3B cultures compared to Huh7 cell cultures. Interestingly, we also observed that interferon stimulated gene (i.e. ISG56) expression was significantly and differentially up-regulated in PLC and Hep3B cells following viral infection.
We conclude that the restrictions observed later during HCV infection in these cell lines could in part be attributed to HCV-induced innate signaling. Nevertheless, the identification of two new cell lines capable of supporting authentic HCVcc infection, even at reduced levels, expands the current repertoire of cell lines amendable for the study of HCV in vitro and should aid in further elucidating HCV biology and the cellular determinants that modulate HCV infection.
Worldwide, between 130 and 170 million individuals are chronically infected with hepatitis C virus (HCV), a positive-strand RNA virus that infects the liver [1, 2]. Although acute infection is typically asymptomatic, ~80% of patients fail to clear the virus resulting in a chronic infection associated with the development of significant liver disease, such as fibrosis, cirrhosis, steatosis, insulin resistance and hepatocellular carcinoma (HCC) . In fact, HCV-related HCC accounts for over 50% of HCC cases and over 30% of liver transplants in the United States. Despite this obvious public health burden, there is no vaccine to prevent infection and current interferon-based treatment options have toxic side effects and limited efficacy.
The main obstacle that has impeded HCV research and antiviral drug development since its discovery in 1989  has been the lack of a robust infectious cell culture system capable of recapitulating all aspects of the viral lifecycle. Although early advancements in the study of HCV were made using surrogate systems , replicons [6–9] and HCV pseudotyped particles (HCVpp) , it was not until the development of the cell-culture derived HCV (HCVcc) system in 2005 that robust HCV infection was finally achieved in vitro [11–13]. This system was based on the identification of an HCV genotype 2a molecular clone , shown to be capable of replicating and assembling infectious particles in cell culture, and the discovery that the human hepatoma Huh7 cell line is permissive for HCV infection. Although numerous other human hepatoma cell lines exist, only HepG2 cells and a few other hepatoma cell lines have been rigorously tested for HCVcc permissiveness to date with varying degrees of success [11, 15–20]. Identification of other cell lines able to support HCV infection would not only expand our current repertoire of cell lines available for the study of HCV, but could also prove useful for the identification of cellular determinants of HCV infection.
To identify other cell lines suitable for HCV infection studies, we assembled a panel of hepatic and non-hepatic cell lines and assessed their permissiveness for HCV infection. Here we show HCVcc infection (i.e. replication, protein translation and de novo virion production) in human hepatoma cell lines PLC/PRF/5 and Hep3B. Like Huh7 cells, PLC cells, a human hepatoma cell line first isolated in the early 1970s  and Hep3B cells, a human hepatoma cell line derived from a hepatocellular carcinoma isolated from an 8 year old male , have been previously utilized for HCV entry (HCVpp) [10, 23–31] studies; however, to our knowledge, HCVcc infection and RNA replication in these two cell lines in the absence of complementation has not been previously reported.
Summary of Cell Lines
Human epithelial colorectal adenocarcinoma
Human embryonic kidney epithelial
Human epithelial carcinoma
Human adrenocortical carcinoma
Chinese hamster ovary
To assess permissiveness for HCVcc infection, all cells were infected with HCVcc at an MOI of 2.0 FFU/cell and intracellular HCV RNA was determined by RTqPCR analysis 72 h p.i. We included Chinese hamster ovary (CHO-K1) cells as they lack all known HCV entry receptors and therefore serve as a control for background HCV RNA levels (i.e. non-specific cell bound HCV) (Figure 1B, dashed line = 102 copies/μg RNA) . As expected, Huh7 cells were highly permissive for HCVcc and replicated HCV RNA to levels of 2.0 × 106 ± 8.2 × 104 copies/μg RNA by 72 h p.i. Caco-2 cell showed minimal to no HCVcc permissiveness, reaching levels of only 4.0 × 107 ± 7.1 × 101 copies/μg RNA. Although Caco-2 cells have previously been reported to support suboptimal HCVcc infection , the low levels of HCV RNA (p value > 0.05) measured in these infected cultures are likely due to receptor-bound HCV similar to that of the non-permissive parental HepG2 cell line. Addition of CD81 to the HepG2 cells conferred HCVcc permissiveness, as previously reported , resulting in increased HCV RNA replication of 1.3 × 104 ± 4.8 × 102 copies/μg RNA (p value < 0.01). Notably, statistically significant HCVcc infection was also detected in PLC cells and Hep3B cells. Although PLC cells were less permissive for HCVpp (Figure 1A), PLC cells contained 10-fold higher HCV RNA levels (3.9 × 104 ± 2.6 × 103 copies/μg RNA) 72 h after infection with HCVcc compared to Hep3B cells (2.8 × 103 ± 3.5 × 102 copies/μg RNA) (Figure 1B), which were as permissive as Huh7 cells for HCVpp infection (Figure 1A). Taken together, these data indicate that PLC and Hep3B cells are permissive for both HCVpp and HCVcc infection, although their permissiveness for HCVcc and HCVpp infection is reduced to different degrees compared to Huh7 cells, suggesting that PLC and Hep3B cells may differ in their capacity to efficiently support specific aspects of the HCV lifecycle. Thus, we initiated experiments to systematically dissect PLC and Hep3B permissiveness for HCVcc infection, focusing separately on each step in the viral lifecycle.
Analysis of HCV-positive cells by immunocytochemical staining of HCV E2 protein 5 days p.i (Figure 5B), indicated that while the majority of cells in the Huh7 culture had become infected, only a small percentage of the cells in the PLC, Hep3B and HepG2-CD81 cultures were infected likely representing the 10% of cells that where initially infected by the viral inoculum. Since viral spread to a large extent is mediated by de novo secretion of infectious HCV virions, we next quantified the level of infectious HCVcc secreted into the supernatants of each infected cell line over the course of 7 days (Figure 5C) using a standard HCV foci formation assay as described . While infectious HCVcc was detectable in Hep3B and HepG2-CD81-infected cultures at reduced levels, infectious HCVcc was undetectable (i.e. below the lower limit of the assay) in the culture supernatant of HCV-infected PLC cells even at day 2 when the PLC cultures had amplified a higher level of intracellular HCV RNA than the Hep3B and HepG2-CD81 cells (Figure 5C).
In this study we characterized a panel of hepatic and non-hepatic cell lines (Table 1) for HCVcc permissiveness. All non-hepatic cell lines were either refractory or marginally permissive for HCVpp and HCVcc infection (Figure 1), as previously shown [10, 25, 30, 32, 35]; however, contrary to commonly held perception, all three of the hepatoma cell lines tested were permissive for HCVcc infection, although to varying degrees relative to Huh7 cells.
Considering the phenotypic differences observed among the hepatoma cell lines (Additional file 1: Figure S2), the perception that Huh7 cells are relatively unique in their ability to support HCV infection [34, 46], and based on previous reports demonstrating varying degrees of HCVcc infection in other hepatoma cell lines, such as HepG2, HepaRG, and immortalized human hepatoma (IHH) cells [15, 16, 18–20, 32, 47], we were surprised that HCVcc infection and replication could be readily detected in both Hep3B and PLC cells (Figure 1). In fact, HCV RNA levels exceeding 104 copies/μg RNA were detected in PLC cells 3 days post infection with HCVcc. When compared directly to Huh7 cells, however, it was apparent that HCVcc infection in both PLC and Hep3B cells was reduced (2.0 × 106 ± 8.2 × 104 vs. 3.9 × 104 ± 2.6 × 103 and 2.8 × 103 ± 3.5 × 102 copies/μg RNA, respectively). In addition, our initial screen also showed notable differences in permissiveness for HCVpp infection between these two cell lines. Specifically, HCVpp infectivity was ~65% lower in PLC cells compared to HCVpp-infected Huh7 and Hep3B cells. However, although significant (p value = 0.03 and 0.02 for JFHpp and H77pp, respectively), we have seen similar variability in permissiveness for HCVpp infection even among fully HCVcc-permissive Huh7 cell lines from different laboratories (Additional file 1: Figure S3 and ), indicating that this level of HCV entry should be sufficient to support robust HCVcc infection. Consistent with this hypothesis, permissiveness for HCVcc infection initiation was notably higher in PLC cells compared to HCV-infected Hep3B cells (Figure 1B and 4B), despite the lower permissiveness of the PLCs for HCVpp entry (Figure 1A). Taken together, the results from our initial screen (Figure 1) indicated that PLC and Hep3B cells are indeed permissive for both HCVpp and HCVcc infection; however, differences in permissiveness compared to Huh7 cells and between each cell line do exist, and thus we initiated a systematic analysis of PLC and Hep3B permissiveness for HCVcc infection, performing experiments that focused on the different steps of the viral lifecycle (i.e. entry, replication, egress and spread).
i. HCV entry. To determine if the differences in HCVpp and HCVcc infection between each hepatoma cell line could be attributed to entry factors already shown to modulate HCV permissiveness in other hepatoma cell lines [25, 32, 48–51], we examined the expression of four essential HCV entry factors (i.e. CD81, SR-BI, CLDN1 and OCLN) by RTqPCR, flow cytometric and immunofluorescence analysis (Figure 2). Interestingly, the data indicated that when compared to the fully permissive Huh7 cell line, no obvious differences in mRNA level or cell surface expression of CD81, SR-BI, CLDN1 or OCLN was observed in PLC, Hep3B or HepG2-CD81 cells. In addition, we over-expressed each of the four HCV entry factors in each cell line since we and others have shown that expression of HCV entry factors in trans can enhance HCVpp and HCVcc entry in cells where HCV permissiveness is low [25, 32, 34]. Consistent with the observation that these cell lines already express the necessary levels of the four HCV entry factors, over-expression of CD81, SR-BI, CLDN1 or OCLN individually or in combination did not significantly increase HCVpp or HCVcc entry in any of the hepatoma cell lines (Figure 3). Hence, the current data indicate that this panel of hepatoma cell lines expresses the minimum set of known entry factors necessary for efficient HCV entry. However, we cannot rule out the possibility that the cells tested are deficient in another HCV entry factor (e.g. the transferin receptor 1 protein  or the Niemann-Pick C1-Like 1 cholesterol absorption receptor , which we recently showed to be HCV entry factors), entry cofactors (e.g. epidermal growth factor receptor and ephrin receptor A2 ) or a post entry host cellular protein required for efficient viral fusion or nucleocapsid uncoating.
ii. HCV RNA replication. To examine HCV replication independent of inherent differences in PLC and Hep3B cell transfection efficiency, we took advantage of the G418-selectable HCVcc G418 virus , which can be used to establish HCV fl2a replicon cells via direct infection of cells rather than electroporation. Using this approach, 88, 77 and 52 G418-resistant colonies were formed in Huh7, PLC and Hep3B cultures, respectively, 3 weeks following infection with 100 FFU of HCVcc G418 (Figure 4B). Additional analysis of HCV RNA replication levels in selected fl2a clones revealed that comparable levels of HCV RNA replication were achieved in all three cell lines (Figure 4D). Likewise similar levels of intracellular HCV RNA were achieved in sg2a replicon cell clones (Figure 4C). Importantly, since G418-resistant colony formation following HCVcc G418 infection is dependent on both successful viral entry and efficient HCV RNA replication, the fact that similar numbers of G418-resistant colonies and equal levels of HCV RNA replication were achieved in both PLC and Hep3B cells, compared to Huh7 cells, indicate that the cumulative efficiency of viral entry plus subsequent RNA replication initiation is relatively equivalent between PLC, Hep3B and Huh7 cells.
iii. Spread and infectious HCVcc production. By performing a 7 day low MOI infection assay, we were able to assess the efficiency of viral spread by assessing intracellular HCV RNA expansion relative to de novo infectious HCVcc production and by visualizing viral spread directly by immunostaining for HCV-positive cells. Analysis of HCV RNA replication following infection of each cell line with HCVcc (Figure 5A) or electroporation with full-length infectious HCV JFH-1 in vitro-transcribed RNA (Additional file 1:Figure S5) revealed that while intracellular HCV RNA initially increased in all the infected/transfected cell cultures at different rates, it was only in Huh7 cultures where HCV RNA levels continued to increase exponentially past day 2 or 3 post infection/transfection. Notably, exponential increase of viral RNA in these cultures after day 2-3 p.i. would require spread of the virus from the original infected/transfected cells. Consistent with this, HCV E2 staining on day 5 post-HCVcc infection revealed that the vast majority of Huh7 cells were HCV-positive while little to no spread was evident in the PLC, Hep3B or HepG2-CD81 cell cultures (Figure 5B). Thus, while infection could be initiated in all these cell lines, only Huh7 cells appeared to support efficient viral spread. Since spread of HCV to naïve cells following infection is dependent on secretion of de novo infectious virions, we measured infectious HCVcc in the supernatant of infected cultures and observed detectable but reduced levels of infectious HCVcc in Hep3B and HepG2-CD81 culture supernatants and undetectable levels of HCVcc in infected PLC cultures (Figure 5C). Low steady-state levels of intracellular HCV RNA and infectious virus production in the Hep3B and HepG2-CD81 cells could result from a defect/bottleneck in any phase of the viral life cycle (e.g. reduced and/or ISG inhibition of entry, replication or secretion); however, since the cumulative efficiency of viral entry plus subsequent initiation of HCV RNA replication appears to be relatively equivalent between Hep3B, HepG2-CD81 and Huh7 cells (Figure 4B), it is reasonable to speculate that robust HCV infection in Hep3B and HepG2-CD81 cells may be limited by a decreased capacity for virus production compared to Huh7 cells. Of course, in the case of PLC cells, there was a clear and severe defect in HCVcc virus production. Not only were no infectious particles detected in the supernatant of infected cultures (Figure 5B and 6A), but analysis of HCVcc present within the cell revealed low to undetectable levels of intracellular infectious virions (Figure 6C) and comparably low levels of encapsidated HCV RNA in both these extra- and intra-cellular samples (Figure 6B and 6D) suggesting virion assembly is restricted at or before genome encapsidation.
The reduced ability of PLC, Hep3B and HepG2-CD81 cell cultures to support robust steady-state infection levels or spread of HCVcc is likely multifactorial and could be directly due to or influenced by the lack of sufficient levels of a cellular protein necessary for efficient production of infectious progeny virus or a consequence of the presence of an inhibitory factor.
i. ISG induction. Since induction of innate immune signaling can have negative affects on multiple steps in the HCV lifecycle, we assessed the ability of PLC, Hep3B and HepG2-CD81 cells to mount an innate immune response against HCV infection by measuring ISG56 mRNA induction, as a representative ISG, following HCVcc infection. Importantly, while no induction of ISG56 was observed in Huh7 cells, as previously published , ISG56 mRNA was up-regulated in HCV-infected PLC, Hep3B and HepG2 cells, with PLC cells exhibiting the most significant induction following HCVcc infection (Figure 7). Although it is generally believed that most cultured hepatoma cells generally are impaired for poly(I-C)- and virus-activated IFN responses , these results are consistent with previous findings that IFN-β promoter activity is more potently induced in HepG2 and Hep3B cells than in Huh7 cells following either liposome-mediated transfection of poly(I-C) or Sendai virus infection . Relevant to this, a more recent publication by Marukian et al.  shows a correlation between innate antiviral gene induction and impaired HCV replication and spread in primary liver cells. Likewise, HCV spread was not observed in highly differentiated microscale primary human hepatocyte cultures described by Ploss et al., (2010), who speculated that while the expression of viral proteins in the initially infected cells might be sufficient to blunt intracellular antiviral signaling and allow sustained viral replication, interferon produced by the infected cell may be sufficient to signal to/activate adjacent naïve cells rendering them resistant to infection and thus limiting subsequent viral spread . Thus, the differences in ISG induction observed between these cells lines (Figure 7) may keep HCV replication lower on a per cell basis (Hep3B and HepG2-CD81) and/or at higher levels successfully inhibit viral replication in the infected cells sufficiently to contribute to clearance of the infection (PLC).
ii. miR-122. While ISGs are well known negative determinants of HCV permissiveness, numerous positive determinants required for efficient HCV replication have also been identified (reviewed in ). Although overlap between independent studies is not often observed, leaving the relevance of many of these factors to be confirmed, new data from multiple laboratories has recently demonstrated that human micro RNA (miR122) is a critical liver-specific factor required for robust HCV infection and secretion [60–65]. Because IFN treatment has been shown to reduce miR122 expression in Huh7 cells , it is possible that the enhanced ISG induction observed in the other three cell lines may more potently reduce this important positive regulator of HCV infection. Likewise, miR122 has been shown to play an important role in regulating cholesterol homeostasis, fatty acid metabolism and lipogenesis [63–65, 67], three lipid metabolic pathways shown to be necessary for HCV replication, assembly and secretion. In fact, just prior to submitting this manuscript, Evans and colleagues and Matsuura and colleagues separately showed that exogenously expressing human miR122 in HepG2 or Hep3B cells, respectively, results in robust HCV replication and infectious virus secretion following HCVcc inoculation or HCV RNA transfection [19, 20]. Hence, lack of adequate miR122 may also contribute to the reduced HCV permissiveness of certain cell lines.
In summary, by testing a panel of human hepatoma and non-hepatoma cells for HCVcc permissiveness we identified new cell lines capable of supporting authentic HCVcc infection (e.g. entry, replication, protein expression and at least for Hep3B cells, de novo virion production). The permissiveness of PLC and Hep3B cells for HCVcc infection is clearly less robust than that achieved in the highly HCVcc-permissive Huh7 cell lines  and while further studies are needed to definitively and quantitatively assess the host cell factors that limit HCV infection in these cells, these two hepatoma cell lines nonetheless provide new in vitro tools for elucidating the cellular factors that control or mediate HCV infection, particularly those associated with HCV ISG induction or those involved in de novo HCVcc production and secretion. In addition, HCV sub-genomic and full-length replicons have not been previously established in Hep3B and PLC cells . Thus, the clones generated in this study add to the current repertoire of sub-genomic and full-length HCV replicons already available to study specific aspects of the HCV life cycle such as HCV polyprotein processing, replication complex formation and HCV RNA replication. Expanding our arsenal of reagents and cell lines amendable for the study of HCV should certainly advance our overall understanding of the HCV viral life cycle and the cellular determinants involved, facilitating the potential development of new and more specific HCV antivirals.
Huh7-1 cells have been previously described . The following cells were purchased from the American Type Culture Collection: PLC/PRF/5 cells (CRL-8024), HepG2 cells (HB-8065), HeLa cells (CCl-2), SW13 cells (CCl-105), and CHO-K1 cells (CCL-61). Hep3B and 293T cells were kindly provided by Dr. Lijun Rong (University of Illinois at Chicago, Chicago, IL) and Caco-2 cells by Dr. Waddah Alrefai (University of Illinois at Chicago, Chicago, IL). All human cell lines were cultured in complete Dulbecco's modified Eagle's medium (DMEM) (Hyclone, Logan, UT). CHO-K1 cells were cultured in Ham's F-12 medium (Gibco Invitrogen, Carlsbad, CA). Media was supplemented with 10% fetal bovine serum (FBS) (Hyclone), 100 units/ml penicillin, 100 mg/ml streptomycin, 2 mM L-glutamine (Gibco Invitrogen) and in the case of HCV replicon cells 500 μg/ml G418 (Invitrogen).
JFH-1 cell culture-propagated HCV (HCVcc) viral stocks were obtained by infection of naïve Huh7-1 cells at a multiplicity of infection (MOI) of 0.01 focus forming units (FFU)/cell, using medium from Huh7-1 cells electroporated with in vitro-transcribed full length infectious HCV JFH-1 RNA as previously described .
The genotype 2a infectious JFH-1 (pJFH-1), the full length (fl) JFH-1 replicon (pFLJFH) and the subgenomic (sg) JFH-1 replicon (pSGJFH) plasmids were kindly provided by Dr. Wakita (National Institute of Infectious Diseases, Tokyo, Japan) and have been previously described [12, 14, 38]. The human CD81 (pEE6-huCD81), human SR-BI (pZeo_hSR-BI), human CLDN1 (pZeo_CLDN1) and human OCLN (pCDNA3.1_OCLN) expression plasmids have been previously described .
Pseudotyped viruses were produced as previously described . Briefly, pseudotyped viruses were generated by co-transfection of DNA vectors encoding HCV or vesicular stomatitis virus (VSV) envelope glycoproteins with an Env-deficient HIV vector carrying a luciferase reporter gene (pNL4-3-Luc-R--E-) into 293T producer cells. The plasmids used for pseudotyped virus generation have been described previously . Supernatants were collected 48 h post transfection, filtered through a 0.45 μm-pore-size filter (BD Biosciences), aliquoted, frozen and subsequently titered using the QuickTiter Lentivirus Titer Kit (Cell Biolabs, Inc., San Diego, CA) according to the manufacturer's instructions.
For infections, cells were seeded 24 h prior to infection in 96-well plates such that cell confluence at the time of infection was 90%. Triplicate wells were inoculated with equal titers of JFHpp, H77pp and VSVGpp for 6 h, washed twice with 1 × PBS following infection, and then overlaid with 200 μl cDMEM. At 72 h p.i. cultures were lysed in 20 μl of lysis reagent to measure luciferase activity (Promega, Madison, WI) using a FLUOstar Optima microplate reader (BMG Labtechnologies Inc, Durham, NC). For all pseudotype virus experiments presented herein, background-corrected (BC) HCVpp RLU values were normalized to corresponding BC-corrected VSVGpp RLU values: [(HCVpp-BC)/(VSVG-BC)].
For infection of cell lines, each cell line was seeded 24 h prior to infection in 96-well plates such that cell confluence at the time of infection was 90%. Triplicate wells were inoculated with HCVcc at an MOI of 2.0 FFU/cell and 72 h p.i. total cellular RNA was isolated for reverse transcription followed by real-time quantitative PCR analysis (RTqPCR). For low MOI HCV RNA kinetic analysis, cells were seeded 24 h prior to infection in 6-well plates such that cell confluence at the time of infection was 80%. Triplicate wells were infected with JFH-1 HCV at an MOI of 0.01 FFU/cell. During the 7 days infection assay, infected cells were trypsinized before reaching confluence and re-plated at a 1:3 dilution to maintain active growth. At indicated times p.i., medium and/or cellular RNA was harvested from triplicate wells for titration or RTqPCR analysis, respectively.
Total intracellular RNA was isolated in 1 × Nucleic Acid Purification Lysis Solution (Applied Biosystems, Foster City, CA) and purified using an ABI PRISM™ 6100 Nucleic Acid PrepStation (Applied Biosystems), as per the manufacturer's instructions. Extracellular RNA from cell supernatants or intracellular HCV RNA from lysed cell pellets was treated with 4.5 units of S7 Micrococcal nuclease (Fermentas, Glen Burnie, MD) for 30 min at room temperature, and nuclease-treated RNA was isolated by the guanidine thiocyanate (GTC) method using 1.6 × GTC containing 2 μg of murine total liver RNA and following standard protocols . One μg of purified RNA was used for cDNA synthesis using the TaqMan reverse transcription reagents (Applied Biosystems), followed by SYBR green RTqPCR using an Applied Biosystems 7300 real-time thermocycler (Applied Biosystems). Thermal cycling consisted of an initial 10 min denaturation step at 95°C followed by 40 cycles of denaturation (15 s at 95°C) and annealing/extension (1 min at 60°C). HCV, human GAPDH, murine GAPDH, human CD81, human SR-BI, human CLDN1, human OCLN and human ISG56 RNA levels were determined relative to standard curves comprised of serial dilutions of plasmids containing the JFH-1 HCV cDNA or the human GAPDH, murine GAPDH, human CD81, human SR-BI, human CLDN1, human OCLN and human ISG56 coding sequences, respectively. The PCR primers used to amplify each respective amplicon were: Universal HCV primers  5'-GCC TAG CCA TGG CGT TAG TA -3' (sense) and 5'- CTC CCG GGG CACTCG CAA GC-3' (anti-sense), human GAPDH  5'-GAA GGT GAA GGT CGG AGT C-3' (sense) and 5'-GAA GAT GGT GAT GGG ATT TC-3' (anti-sense), murine GAPDH  5'-TCT GGA AAG CTG TGG CGT G-3' (sense) and 5'-CCA GTG AGC TTC CCG TTC AG-3' (antisense), human CD81  5'-ACC TCC TGT ATC TGG AGC TGG-3' (sense) and 5'-TTG GCG ATC TGG TCC TTG TTG-3' (anti-sense), human SR-BI  5'-TCG CAG GCA TTG GAC AAA CT-3' (sense) and 5'-CTC CTT ATC CTT TGA GCC CTT TT-3' (anti-sense), human CLDN1  5'- GTG GAG GAT TTA CTC CTA TGC CG-3' (sense) and 5'- ATC AAG GCA CGG GTT GCT T-3' (anti-sense), human OCLN  5'- TCA AAC CGA ATC ATT ATG CAC CA-3' (sense) and 5'- AGA TGG CAA TGC ACA TCA CAA-3' (anti-sense), and human ISG56  5'- GGG CAG ACT GGC AGA AGC -3' (sense) and 5'- TAT AGC GGA AGG GAT TTG AAA GC -3' (anti-sense).
Cells were resuspended in 150 μl of FACS buffer (1 × PBS containing 2% (v/v) FBS, 0.3% (w/v) NaN3 and 1 mM EDTA) and incubated for 60 min at 4°C with a 1:100 dilution of antibodies specific for CD81 (AbD Serotec) or SR-BI (BD BioSciences) Following three rinses with FACS buffer, bound antibodies were detected by incubation for 1 h at 4°C with an phycoerythrin (PE)-conjugated anti-mouse (BD Pharmingen) antibody at a dilution of 1:200. Cells stained with an irrelevant mouse immunoglobulin G (IgG) antibody and respective PE-conjugated secondary antibody served as negative controls. Cells were washed three times, fixed in FACS buffer containing 4% (w/v) PFA, and analyzed by flow cytometry using the DakoCytomation CyAn system (Dako, Carpinteria, CA) and Summit Software v4.3 (Dako).
Cells were fixed with 4% PFA (Sigma, St. Louis, MO) at indicated times and immunofluorescence analysis was performed as previously described . Briefly, fixed cultures were rinsed three times with 1 × PBS, permeabilized with 50% Methanol/50% acetone (v/v) (Fisher) and subsequently blocked for 1 h with 1 × PBS containing 3% (w/v) bovine serum albumin (BSA) (Sigma) and 10% (v/v) FBS. Cells were stained with a 1:750 dilution of a mouse anti-human CLDN1 (Abnova, Taipei, Taiwan) or mouse anti-human OCLN (Zymed, San Francisco, CA) primary antibody overnight at 4°C, followed by incubation with a 1:750 dilution of an anti-mouse Alexa-555 conjugated secondary antibody (Molecular Probes) for 1 h at room temperature. Cell nuclei were stained by Hoechst dye. Bound antibodies were visualized via confocal microscopy (630X, Zeiss LSM 510, Germany) and compared to negative control samples stained with an irrelevant mouse control antibody (Santa Cruz Biotechnology) and Alexa-555 conjugated secondary antibody. Images were analyzed using Zeiss LSM Alpha Imager Browser v4.0 software (Zeiss), and brightness and contrast were adjusted using Adobe®Photoshop® (San Jose, CA).
HCV sg and fl 2a replicons were established as previously described . Briefly, 1 μg of in vitro-transcribed HCV genotype sg2a or fl2a replicon RNA was transfected into cells using a modified electroporation protocol . Transfected cells were diluted 1:500, seeded in 100 mm tissue culture dishes and maintained in the presence of G418 (Invitrogen) at a concentration of 500 μg/ml until all cells died or distinct G418-resistant cell colonies formed. To visualize colony formation, cells were fixed with ethanol and stained with crystal violet. Alternatively, colonies were expanded to establish replicon cell lines. HCVcc G418 was harvested from stable fl 2a Huh7 replicon cells and infectivity titers were determined as described below.
Culture supernatants were serially diluted 10-fold and used to infect 96-well Huh7 cultures. At 24 h p.i., cultures were overlayed with complete DMEM containing a final concentration of 0.25% methylcellulose (Fluka BioChemika, Switzerland). Seventy-two hours p.i., cells were fixed in 4% paraformaldehyde (Sigma), and immunohistochemically stained for HCV E2 using a human monoclonal anti-E2 antibody C1  (a gift from Drs. Mansun Law and Dennis Burton, The Scripps Research Institute) as described . Viral titers are expressed as FFU/ml, determined by the average E2-positive foci number detected at the highest HCV-positive dilution.
To quantify intracellular HCVcc, HCV-infected cell cultures were washed three times with 1 × PBS, trypsinized for 5 min at room temperature and cells resuspended in 1 ml of 10% cDMEM. Cells were pelleted at 1,400 RPM for 5 min at 4°C, frozen and then thawed three times using a 95% ethanol:dry ice bath. Samples were then centrifuged at 1,400 RPM for 5 min at 4°C to remove cell debris. The supernatant fractions were used for titration of infectious HCVcc or for HCV RNA analysis, as described above.
Data are presented as the means ± standard deviation (SD). Significant differences were determined by one-way analysis of variance (ANOVA) followed by Tukey's post hoc t test (GraphPad Prism© Software).
Hepatitis C virus
Japanese Fulminant Hepatitis
Hepatitis C virus cell-cultured produced
HCV pseudotype particles
Vesicular stomatitis virus G protein pseudotype particles
Multiplicity of infection
Focus forming units
Real-time quantitative PCR
Scavenger receptor class B member I
Interferon stimulated gene.
The authors graciously thank Drs. Lijun Rong and Waddah Alrefai (University of Illinois at Chicago) for providing Hep3B, 293T and Caco-2 cells and Dr. Giorgos Koutsoudakis and the entire Uprichard Lab for helpful discussion. This work was supported by the National Institutes of Health Public Health Service Grants R56/R01-AI078881 and R21-CA133266 and the University of Illinois Chicago Council to support Gastrointestinal and Liver Disease (UIC GILD).
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