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Abstract

Persistent infections with human immunodeficiency virus type 1 (HIV-1) and hepatitis C virus (HCV) are a major cause of morbidity and mortality worldwide. As sentinels of our immune system, dendritic cells (DCs) play a central role in initiating and regulating a potent antiviral immune response. Recent advances in our understanding of the role of DCs during HIV-1 and HCV infection have provided crucial insights into the mechanisms employed by these viruses to impair DC functions in order to evade an effective immune response against them. Modulation of the immunological synapse between DC and T-cell, as well as dysregulation of the crosstalk between DCs and natural killer (NK) cells, are emerging as two crucial mechanisms. This review focuses on understanding the interaction of HIV-1 and HCV with DCs not only to understand the immunopathogenesis of chronic HIV-1 and HCV infection, but also to explore the possibilities of DC-based immunotherapeutic approaches against them. Host genetic makeup is known to play major roles in infection outcome and rate of disease progression, as well as response to anti-viral therapy in both HIV-1 and HCV-infected individuals. Therefore, we highlight the genetic variations that can potentially affect DC functions, especially in the setting of chronic viral infection. Altogether, we address if DCs’ potential as critical effectors of antiviral immune response could indeed be utilized to combat chronic infection with HIV-1 and HCV.

Keywords

dendritic cells HIV-1 HCV HIV-1/HCV co-infection human chronic viral infections DC-NK cell crosstalk innate immune response antigen-specific immune response

Introduction

The immune response generated during a viral infection involves a complex interplay between the virus and the two arms of the immune system, innate and adaptive. Dendritic cells (DCs) are a specialized category of professional antigen-presenting cells (APCs) that act as messengers between the innate and the adaptive immune system.¹ Immature DCs are derived from hematopoietic bone marrow progenitor cells and are widely distributed within tissues such as the skin, mucosal surfaces, and blood that come in direct contact with the external environment. DCs are equipped with pattern recognition receptors (PRRs) such as Toll-like receptors (TLRs), whose role is to sense a wide array of pathogen-associated molecular patterns (PAMPs). In humans, the TLR family consists of 10 members, named TLR1-10, with each member being specific for the PAMP it recognizes; TLR7, for example, recognizes single-stranded RNA and TLR3 recognizes double-stranded RNA.¹ Plasmacytoid DCs (pDCs) express TLR7 and TLR9, whereas myeloid DCs (mDCs) express TLR1-3 and TLR8.² Upon TLR-mediated viral sensing, DCs get activated and migrate to lymph nodes where they prime a naive T cell against the viral peptide that is presented on their surface by MHC molecules. DCs can process both extracellular antigens via the lysosomal pathway and intracellular proteins via the proteasomal pathway.³ After viral processing, DCs become activated and migrate to the draining lymph nodes, where they transform into mature DCs in the T-cell-rich areas. Maturation of DCs involves several changes including cytoskeleton reorganization, redistribution of MHC molecules from endocytic compartments to the surface, inhibition of antigen uptake, and an increase in the expression of co-stimulatory and adhesion molecules as well as chemokine receptors.⁴

DCs exhibit heterogeneity at several levels including phenotype, function, and anatomical location.⁵ DCs in the epidermis are referred to as Langerhans cells (LCs), dermal DCs are found in dermis, and interstitial DCs are found in all peripheral tissues except skin. Blood DCs in turn are broadly classified into two major groups, mDCs and pDCs, with mDCs being further comprised of different subsets. Table 1 summarizes the phenotype and functional characteristics of various DC subsets, clearly indicating a low frequency of DCs in blood. To facilitate ex vivo analysis of blood DCs, we have recently developed an antibody cocktail for polychromatic flow cytometry and evaluated its applicability for immune profiling of human T-cell leukemia virus type 1 (HTLV-1), as well as HIV-1/ HCV co-infected patient cohorts. These observations remain unpublished. We have also demonstrated the suitability of using this newly developed cocktail in immunological investigations of frozen peripheral blood mononuclear cells (PBMCs) from infected patients. The use of multi-parametric antibody cocktails has been proven to be very useful in assessing the frequency as well as phenotypic and functional changes on rare DC subsets during viral infections.

Table 1.

Frequency and phenotype of blood DC subsets.

Subset	Marker	% of PBMCs	Phenotypic markers	TLRs	Cytokine production
Plasmacytoid DCs
CD303⁺ DCs	CD303 (BDCA2) CD304 (BDCA4)	~0.2	CD1c⁺, CD11c^–, CD16^–, CD45RA⁺, CD88^–, C3aR^–, CD123⁺	TLR7, TLR9	High IFNα
Myeloid DCs
CD1c⁺ DCs	CD1c	~0.4	CD33⁺, CD13⁺, CD11b⁺, CD1c⁺, CD11c⁺, CD16^–, CD45RA^–, CD88^– (C5aR), C3aR^–, CD123^low	TLR1, TLR2 TLR3, TLR4	Low TNFα and IL12p70
CD141⁺ DCs	CD141 (BDCA3)	~0.05	CD1c^–, CD11c^low, CD16^–, CD45RA^–, CD88^–, C3aR^–, CD123^–	TLR3	High IL12p70 and IFNβ
slanDCs	6sulfoLacNAc²⁶⁰	~1.2	CD1c^–, CD11c⁺, CD16⁺, CD45RA⁺, CD88⁺, C3aR⁺, CD123^low	TLR4	High TNFα and IL12p70

Different DC subsets have acquired both distinct and overlapping roles in the immune system.⁶ Figure 1 illustrates the role of DCs in initiating and regulating the adaptive immune response. Activated mDCs are responsible for priming CD4⁺ and CD8⁺ T cells against a specific pathogenic epitope. In addition, they produce interleukin (IL)-12 and IL-15, both of which activate natural killer (NK) cells and promote the differentiation of epitope-specific CD4⁺ T-helper (T_H) cells and CD8⁺ T cells into T_H1 cells and cytotoxic T lymphocytes (CTLs) respectively. Activated NK cells have two major roles. The first role is to secrete interferon-γ (IFNγ), which inhibits viral replication in infected cells. Secondly, NK cells kill virus-infected cells directly through the release of cytolytic mediators such as granzyme. T_H1 cells also secrete IFNγ, which stimulates the activation of CTLs and the production of neutralizing immunoglobulin G2a antibodies by plasma cells. In contrast to mDCs, whose main role is to prime T cells against the virus, pDCs function as one of the earliest mediators of antiviral immune response by producing large amounts of type I IFNs (IFNα and IFNβ) upon viral sensing. Besides inducing an antiviral state in virus-infected cells, type I IFNs take part in activation of NK cells⁷ and promotion of CD4⁺ and CD8⁺ T-cell differentiation and survival.⁸ In addition, pDCs have also been shown to act as APCs.^9–11 Interestingly, recent data suggests that pDCs can facilitate CD4⁺ T_H cell responses to persistent viruses independently of direct antigen presentation,^{12
13} necessitating the need to assimilate enough knowledge about the role of pDCs in antiviral immune response.

Figure 1.

Role of DCs in the antiviral immune response.

The importance of DCs in resolving viral infection has been shown for several viruses including human respiratory syncytial virus and influenza virus.^{14, 15} Our group is focused on gaining complete understanding of the role of DCs in chronic viral infections caused by HTLV-1, HIV-1, and HCV.^16–28 Many studies including ours strongly suggest that DCs play an important role in the control of HCV and HIV infection, two of the most common and fatal blood-borne viruses. Patients in whom HCV infection clears spontaneously or in whom HIV-1 infection is controlled have strong multi epitope-specific CD4⁺ and CD8⁺ T-cell responses; these responses probably reflect the efficient antigen presentation and T-cell activation potential of DCs.^{29, 32} However, the chances of viral clearance after HCV and HIV-1 infection are low, owing to the remarkable ability of these viruses to evade the host immune response and establish chronic infection.

Chronic HIV-1 infection causes acquired immunodeficiency syndrome,³³ which is characterized by severe immunosuppression and associated opportunistic infections.³⁴ According to a recent report by the Joint United Nations Programme on HIV/AIDS, an estimated 33.4 million people around the world are living with HIV infection.³⁵ The Centers for Disease Control and Prevention (CDC) estimated that 1,178,350 persons aged 13 and older were living with HIV infection in the United States as of 2008.³⁶ In 2009, there were an estimated 48,100 new HIV infections.³⁷ Chronic HCV infection causes chronic liver disease and its associated complications such as liver cirrhosis, liver failure, and hepatocellular carcinoma.³⁸ According to the latest update by the World Health Organization (WHO), about 170 million people are chronically infected with HCV and more than 350,000 people worldwide die from HCV-related liver disease each year.³⁹ Figure 2 outlines the outcome and the course of disease progression during HCV infection. It also outlines important factors such as gender, age, ethnicity, and host genetic makeup that favor spontaneous clearance of HCV infection. Apart from HIV-1 and HCV mono-infected patients, a significant population of co-infected patients exists. Overall, co-infection with HCV is found in 30% of HIV-infected patients and in 60% to 90% of HIV-infected injection drug users.^40–42

Figure 2.

Outcome of acute HCV infection.

A weak and narrowly focused antiviral T-cell response is a common denominator in both HIV-1 and HCV infections. Being one of the key players involved in initiation and regulation of the antiviral immune response, DCs are the ideal targets for HIV-1 and HCV to exercise their immune evasion strategies. Therefore, in order to develop novel therapies against chronic HIV-1 and HCV infection, there is a need to understand the interaction between DCs and both these viruses. This review discusses the mechanisms by which HIV-1 and HCV are able to interfere with the normal immune response of the host. We also highlight the role of host genetic variations in modulating various DC functions associated with antiviral immunity. Finally, we discuss the recent advances in the field of anti-HCV drugs.

Do HIV-1 and HCV Infect DCs?

The presence of DCs in the skin and blood as well as at the mucosal surfaces, and their proficiency in antigen uptake, predisposes them to be the primary targets for viruses. Therefore, it is possible that HIV-1 and HCV infect DCs. Replication of the viral genome along with the expression of viral proteins in DCs might interfere with many signaling pathways in DCs, leading to impairment of DC functions and thus rendering them incapable of stimulating a proper T-cell response against the virus. For example, ICP47 of herpes simplex virus 1 and US6 of human herpes virus 5 are known to inhibit the loading of antigenic peptides onto MHC class I molecules, leading to a reduced ability of infected DCs to prime naïve T cells efficiently.⁴³

HIV-1

The main target cells for HIV-1 are mononuclear leukocytes bearing CD4 and the chemokine receptors CC-chemokine receptor 5 (CCR5) and CXC-chemokine receptor 4 (CXCR4);^44–48 however, LCs, pDCs, and mDCs have also been reported to be susceptible to HIV-1 infection.^49–61 HIV-1 replication is generally less productive in DCs than in CD4⁺ T cells,^{49,57,59,62–64} and the frequency of HIV-1-infected DCs in the blood has been reported to be 10 to 100 times lower than that of CD4⁺ T cells.⁶⁵ Immature DCs are more susceptible to HIV-1 infection than mature DCs,⁶⁶ perhaps partly as a result of their higher antigen uptake capacity. Interestingly, replication of HIV-1 in pDCs was found to increase substantially following CD40 ligation.⁶⁷ CD40 is a co-stimulatory molecule found on APCs and its binding to CD40 ligand (CD40L) on T_H cells activates APCs to perform a variety of functions. Thus, HIV-1 replication in pDCs may be upregulated through its interaction with activated CD4⁺ T cells in the extrafollicular zones of the lymphoid tissue.

HCV

Hepatitis C virus primarily infects and replicates in hepatocytes; however, evidence is accumulating about extrahepatic replication of HCV, especially in PBMCs. The highly conserved 5’ untranslated region of HCV RNA has been shown to vary between PBMCs and plasma in the same individual,^68,69 suggesting that HCV alters its replication inside non-hepatic cells. Lymphoid cells may act as HCV reservoirs, thus contributing to the establishment of chronic infection. Different studies have shown low levels of HCV RNA in serum and lymphoid cells after spontaneous or IFN/RBV-induced resolution of chronic hepatitis C.^70,71 In patients with a sustained virological response, small quantities of HCV RNA have been shown to persist in the liver or in PBMCs for up to 9 years.⁷¹ HCV may persist and replicate in the liver and PBMCs of healthy, anti-HCV antibody positive, serum HCV RNA-negative patients who have persistently normal alanine amino transferase levels.⁷² This could present a potential risk for reactivation, especially in the case of immunosuppression due to the presence of HIV-1 infection in the same individual. In fact, HCV RNA in peripheral blood cell subsets in HIV/HCV co-infected patients at the end of IFN/RBV treatment is associated with virological relapse.⁷³ Interestingly, HCV RNA has been shown to reemerge in apparent sustained virological responders receiving immune suppressive therapy.^74,75 This suggests that HCV persists years after IFN/RBV- induced resolution from plasma and suggests that continued immune surveillance is required to prevent its recurrence, even in sustained virological responders.⁷⁴ As far as DCs are concerned, HCV genomic RNA has been detected in mDCs and pDCs isolated from the blood of HCV-infected patients.^76,77 One study, which used strand-specific semi quantitative reverse transcription polymerase chain reaction, has shown that 3 out of 24 HCV-infected patients had DCs carrying the replicative intermediate of HCV.⁷⁶ More such studies are needed to clearly establish whether HCV replicates in blood DCs of infected patients. In one study, monocyte-derived DCs (MDDCs) from healthy donors were found to contain HCV replicative intermediate when incubated with the serum of HCV-infected patients.⁷⁸ This study provides evidence that DCs can at least support the first steps of the viral life cycle. However, other studies wherein MDDCs and various blood DC subsets were incubated with infectious recombinant HCV were not successful in detecting viral replication or viral protein synthesis.^{79, 81}

In summary, DCs can support HIV-1 replication, although at a level much lower than CD4⁺ cells (primary targets for HIV-1); additionally, they cannot support the production of HCV virions, even though HCV may be able to infect DCs and initiate its replication. Many explanations are possible. Firstly, as professional APCs, DCs might degrade the virus in intracellular compartments before it completes its replicative cycle. DC-specific ICAM-3 (intercellular adhesion molecule-3) grabbing non integrin (DC-SIGN or CD209) is a C-type lectin receptor (CLR)^82,83 that has been shown to promote uptake and presentation of HIV-1 by MHC class I and class II molecules.⁸⁴ Scavenger receptor class B member 1 (SRB1) has been shown to mediate in HCV uptake and presentation.⁸⁵ The second possibly explanation involves the fact that host factors required for HIV-1 and HCV replication might be missing in DCs, or DC-specific host factors might restrict HIV-1 and HCV replication. For example, cellular factors such as cytidine deaminase APOBEC3G (apolipoprotein-B mRNA-editing enzyme, catalytic polypeptide-like 3G),^86,87 the transcription factor NFAT (nuclear factor of activated T cells),⁸⁸ the nuclear factor-κB (NF-κB) regulating protein (MURR1),⁸⁹ and polypyrimidinetract-binding protein (PTB)⁹⁰ have been shown to block HIV-1 replication after its entry into resting CD4⁺ T cells, although the relevance of these cellular restriction factors in DCs is not fully studied. Expression levels of APOBEC3G have been shown to correlate with resistance of mDCs to HIV-1.⁹¹ APOBEC3G upregulation by IFNα has been shown to restrict HIV-1 infection in pDCs.⁹² Additionally, engagement of the receptors CCR5 and CD40 with CCL3 and CD40L respectively enhances the expression of APOBEC3G in DCs through activation of the ERK 1/2 and p38 MAP kinase signaling pathways. The third possible explanation is that DCs express low levels of HIV-1 receptor CD4, as well as co-receptors CCR5 and CXCR4.⁹³ HCV co-receptor claudin1 is also present at low levels in DCs.⁸¹ HIV-1 and HCV entry receptors are reviewed in the next section.

HIV-1 uptake by DCs has been shown to trigger TLR8 (via ssRNA), which results in phosphorylation of RNA Polymerase II (RNAPII) at serine 2 of the C-terminal domain (CTD).⁹² On the other hand, binding of HIV-1 envelope protein gp120 with DC-SIGN results in the activation of Raf-1 and ultimately leads to phosphorylation of p65 at serine 276. This modification on p65 recruits positive transcription elongation factor b (p-TEFb) to the long terminal repeat (LTR), which phosphorylates RNAPII at serine 5 of CTD.⁹² It has been shown that phosphorylation of RNAPII at both serine 2 and serine 5 of its CTD promotes full-length transcription of the integrated HIV-1 genome and production of HIV-1 proteins. Thus, HIV-1 induces innate signaling by TLR8, as well as DC-SIGN, and that allows it to cause productive infection of DCs. Despite this, the frequency of blood DCs productively infected with HIV-1 is low. This could be due to increased migration of these DCs from blood to lymph nodes or due to increased rate of apoptosis. Interestingly, HCV glycoprotein E2 is known to interact with DC-SIGN⁹⁴ and this interaction has been shown to activate p38 MAPK pathway, possibly leading to activation of Raf-1. Therefore, it would be interesting to study whether HCV can augment HIV-1 replication in DCs during HIV-1/HCV co-infection.

Role of DCs in Viral Dissemination

Following antigen uptake and activation, DCs present in peripheral tissues migrate to secondary lymphoid organs and present the antigen to the naive T cells. It is therefore not unreasonable to propose that various viruses would exploit this migratory property of DCs in order to disseminate to sites that are favorable for their replication. Herein, we review the entry and recognition of HIV-1 and HCV into DCs.

HIV-1

As some of the first target cells that encounter HIV-1 at the mucosa, DCs contribute to the initial stages of HIV-1 infection and dissemination.^95,96 HIV-1 has been shown to inhibit the fusion between endosomes and autophagosomes, which not only leads to prevention of autophagy-mediated viral degradation and subsequent presentation of viral antigens, but also enhances the survival of HIV-1 inside DCs.^97–100 Enhanced survival of HIV-1 is likely to promote its dissemination to T cells by various mechanisms. Binding and internalization of HIV-1 by DCs is mediated by HIV-1 entry receptor CD4 and co-receptors CCR5 and CXCR4, which are known to be expressed on the surface of DCs.^101,102 Other chemokine receptors that are also suggested to participate in HIV-1 entry are CCR3, CCR8, CCR9, and CXCR6.^96,103 In addition, DCs express C-type lectins such as DC-SIGN, langerin (also known as CLEC4K or CD207), and DC immunoreceptor (DCIR; also known as CLEC4A), which bind to HIV-1.^96,104 Expression of these receptors depends on the DC subtype, activation state, and localization. Even though pDCs express C-type lectins such as BDCA2, binding of HIV-1 to pDCs is generally mediated by interaction of HIV-1 envelope protein gp120, with CD4 expressed on pDCs. Interestingly, the identity of receptors involved in virus-DC interaction seems to affect the fate of virus after its binding to the cell surface. The interaction between the carbohydrate recognition domain of DC-SIGN and gp120 results in internalization of HIV-1 into non-lysosomal compartments in DCs, where it does not undergo degradation. The internalized virion can then be transported within DCs before finally getting transferred to T cells in a process known as transinfection. This model of DC-dependent infection of CD4⁺ T cells, commonly referred to as the Trojan horse model, involves endocytosis of HIV-1 virion by DCs followed by its transmission to the T cells via vesicular exocytosis across the infectious synapse. This structure is analogous to the immunological synapse formed between DCs and T cells in the T-cell areas of lymphoid tissue.¹⁰⁵ A conflicting study,¹⁰⁶ however, demonstrated that transinfected HIV-1 was fully sensitive to surface-applied soluble CD4, which has been shown to inactivate HIV-1 and inhibit its entry even after the virus was sequestered within the DCs. This phenomenon suggests that the sequestered, internalized HIV-1 virions are targeted for degradation and only the surface-bound virions participate in transinfection. A careful reexamination of these observations in a different study¹⁰⁷ showed that mature DCs concentrate viral particles within membrane folds, making them accessible for surface-applied soluble CD4. This suggests that soluble surface-applied CD4-induced reduction in transinfection could be due to inactivation of sequestered HIV-1 virions and that sequestered, internalized HIV-1 could participate in transinfection.

The binding of HIV-1 to DC-SIGN enhances the formation of infectious synapse; the engagement of DC-SIGN by HIV-1 activates Cdc42 and induces membrane extensions in immature DCs, thus facilitating viral propagation across the infectious synapse. It has also been observed that CD4⁺ T cells participate in transinfection by extending membrane protrusions into the virus-containing pockets on DCs. This helps the virus to emerge from the pocket by engaging CD4 on the membrane protrusions. DC-SIGN-independent mechanisms are also involved in DC-mediated HIV-1 transinfection of CD4⁺ T cells.^108–113 Recent data indicates that immature DC-mediated HIV-1 transinfection is partially dependent on DC-SIGN, whereas mature DC-mediated HIV-1 transmission to different target cells is independent of DC-SIGN and C-type lectins.¹¹⁴ However, another study has shown why interaction of HIV-1 with DC-SIGN may be important for efficient HIV-1 transmission. Clusterin (an apolipoprotein) in semen is differentially glycosylated compared to clusterin in blood. Clusterin in semen is a DC-SIGN ligand and can therefore block the interaction between HIV-1 and DC-SIGN, thereby preventing HIV-1 transmission to CD4⁺ T cells. This may also explain why exposure to HIV-1 through sexual contact is less likely to result in infection compared to blood-borne exposure.¹¹⁵

It is known that maturation of DCs increases their efficiency in transmitting HIV.^{56,106,107,114,116–121} DC maturation leads to an upregulation in ICAM-1 (CD54) gene expression, which correlates with mature DC-enhanced transmission of HIV-1 to CD4⁺ T cells.¹²⁰ Interactions between ICAMs and their ligands on T cells can thus be proposed to facilitate DC-T-cell contact and HIV-1 transmission. In fact, it has been shown that ICAM-1 (but not ICAM-2 or −3) is important for DC-mediated HIV-1 transmission ¹²² and that blocking ICAM-1 on DCs impairs HIV-1 transmission.¹²⁰ Because the interaction between ICAM-1 and leukocyte function-associated molecule 1 (LFA-1) is important for DC-T-cell adhesion,¹²³ it has been proposed that the interaction between ICAM-1 on DCs and LFA-1 on CD4⁺ T cells is important for HIV-1 transinfection.¹²⁰ As mentioned previously, HIV-1 can also infect DCs, although less efficiently than CD4⁺ T cells. Many reports have indicated that infected DCs can aid in HIV-1 dissemination by transmitting the viral progeny to T cells; this process is known as cisinfection.^121,124 Interestingly, HIV-1-infected MDDCs show Nef-induced downregulation of CD4 that correlates with enhanced viral transmission.¹²⁵ These results suggest that CD4, which is present at various levels in DC-SIGN-positive primary cells, could be one of the key regulators of HIV-1 transmission.

It is also important to understand the role of different DC subsets in HIV-1 transmission. pDCs are less efficient than mDCs in viral transmission.¹²⁶ LCs also appear to transinfect HIV-1 through surface exposed structures similar to those in mature DCs.^106,116 However, one study suggested that expression of CLR langerin on LCs acts as a barrier to HIV-1 transmission.¹²⁷ Because different mDC subsets have been shown to transfer HIV-1 to activated CD4⁺ T cells,⁹⁶ the question of whether LCs can do so needs to be resolved.

HCV

The idea that DCs might play an important role in dissemination of HCV, a hepatotropic virus, is still in its infancy. HCV envelope protein E2, serum of HCV-infected patients, and retroviruses that are pseudotyped with HCV envelope proteins have all been shown to bind specifically to DC-SIGN.^94,128,129 Therefore, it is possible that DC-SIGN mediates the binding of blood DCs or hepatic DCs in liver sinusoids to the circulating HCV particles. MDDCs expressing DC-SIGN were shown to bind HCV pseudovirus and transmit it efficiently when co-cultured with the human hepatocellular carcinoma cell line Huh7; Huh71 is a cell line that is widely used to study HCV pseudovirus entry as well as productive replication of recombinant infectious HCV.^129,130 Importantly, HCV virus-like particles were shown to bind DC-SIGN and get targeted to nonlysosomal compartments within MDDCs. These particles were thus protected from lysosomal degradation, suggesting that, similar to HIV-1, HCV might also escape the antigen processing and presentation pathways in DCs.¹³¹ HCV bound to blood DCs or hepatic DCs in liver sinusoids may allow the transfer of the virus to the underlying hepatocytes when DCs traverse the sinusoidal lumen in order to gain entry to the hepatic lymph. Beside DCs, liver sinusoidal endothelial cells (LSECs) have also been shown to bind recombinant HCV via interaction of HCV glycoprotein E2 with DC-SIGN and DC-SIGN-related protein (DC-SIGNR or CLEC4M) expressed on the surface of LSECs.¹³² However, LSECs have been found to be non-permissive to the entry of HCV pseudovirus, as well as cell culture-derived HCV.¹³² Nonetheless, high-affinity binding of HCV to LSEC might still be an important initial step towards its efficient entry into the underlying hepatocytes.

Impact of Chronic HIV-1 and HCV Infection on DCs

Dendritic cells are responsible for orchestrating a successful immune response against viruses; viral persistence might therefore be facilitated by its successful impairment of DC functions. At the primary level, viruses can modulate the frequency of various DC subsets by causing their aberrant trafficking, inducing apoptosis, or interfering with their development. Compared with uninfected individuals, HIV-1-infected^60,133–137 as well as HCV-infected^138–143 individuals have lower numbers of mDCs and pDCs. During HIV-1 infection, pDCs migrate to the inflamed lymph nodes, where they become activated, apoptotic, and, frequently, infected with the virus.^144,145 During HCV infection, blood DCs are enriched in the liver,^142,146,147 suggesting that increased migration of DCs to the liver, which is the primary site of HCV replication, causes the observed drop in blood DC count. Other possibilities are that HCV targets DC precursors, as reported by Sansonno et al,¹⁴⁸ or that HCV directly targets DCs to reduce their numbers. In this regard, it has been shown that HCV core, NS3, and NS5 proteins induce apoptosis in mature DCs in vitro.¹⁴⁹ Interestingly, in vitro studies have shown that HCV envelope glycoprotein E2, as well as sera from HCV-infected patients, inhibits the migration of DCs towards CC-chemokine ligand 21 (CCL21), a CCR7 binding chemokine that is important for their homing to lymph nodes.¹⁴² This leads us to an intriguing hypothesis that HCV impairs the ability of DCs to migrate to the draining lymph nodes, causing them to get trapped in the liver. This hypothesis has not been thoroughly investigated in vivo.

Under different immunological states, DCs can either produce IL-12 or IL-10. While IL-12 promotes the differentiation of CD4⁺ and CD8⁺ T cells to T 1 cells and CTLs respectively, IL-10 is capable of inhibiting the same.⁶ MDDCs, mDCs, and pDCs from HIV-1-infected^{150, 152} and HCV-infected^{141
143
153
154} individuals have been shown to upregulate IL-10 and downregulate IL-12 and IFNα production in response to various maturation stimuli (Fig. 1). Furthermore, the ability of NK cells to mediate early antiviral defense might be affected by dysregulated production of cytokines by DCs. Evidence from several studies indicates that defective pDC function during HIV-1 infection contributes towards impaired NK cell activity, particularly their ability to secrete IFNγ.^155,156 Dysregulation of DC-NK cell crosstalk during HIV-1 and HCV infection is discussed in later sections of this study.

Compared to uninfected individuals, DCs isolated from individuals infected with HIV^{150
152} and HCV^{141
157
159} were found to be less efficient in stimulating T-cell activation and proliferation, as seen in mixed lymphocyte reaction. This inefficient allogenic T-cell stimulation by DCs isolated from HIV-1⁹⁹ and HCV-infected¹⁵⁹ patients could be reversed by neutralization of IL-10, suggesting that virus-induced production of IL-10 by DCs could skew the immune response towards tolerance by limiting T-cell activation and proliferation. To gain a different perspective on the impact of HIV-1 and HCV on DCs, various studies have investigated DC function and patients before and after antiviral therapy. Highly active antiretroviral therapy for treating HIV-1 infection has been shown to restore pDC count as well as IFNα production to normal levels.^{155
160} Similarly, in HCV-infected patients that were able to clear the virus upon IFN/RBV treatment, the frequency of pDCs increased substantially and ultimately reached levels observed in uninfected controls.¹⁶¹

Molecular Basis of Virus-DC Interaction

To understand the molecular mechanisms of interaction between these two viruses and DCs, various in vitro studies have used DC subsets isolated from uninfected individuals and exposed them directly to the¹⁶² recombinant infectious virus or viral proteins. Unlike HIV-1 and many other viruses such as influenza virus and herpes simplex virus 1, recombinant and serum-derived HCV have been shown to be poor inducers of IFNα production in pDCs. This suggests that HCV might inhibit IFNα production by pDCs as a strategy to escape IFNα-mediated immune response against itself. In pDCs, TLR7 and TLR9 are endosomal TLRs, responsible for detecting viral RNA and DNA, respectively. Detection of viral RNA or DNA leads to the activation of NF-κB and IFN-regulatory factors, which control the transcription of type I IFNs (IFNα, IFNβ) and various pro-inflammatory cytokines. HCV inhibits IFNα production induced by CpG oligodeoxynucleotide (a TLR9 agonist), but not by resiquimod (a TLR7 agonist).^{79, 80, 164} HIV-1 is also known to impair IFNα production by pDCs, indicating that impaired production of IFNα by pDCs might be a common strategy employed by many viruses to establish a persistent infection. Hepatitis B virus envelope protein HBsAg and HIV-1 envelope protein gp120 have been shown to impair TLR9- mediated IFNα production through binding to a C-type lectin, blood DC antigen 2 (BDCA2, also known as CLEC4C).^162,163 HCV core particles and recombinant noninfectious HCV particles composed of HCV core⁷⁹ and envelope glycoproteins E1 and E2^79,80,164 have been shown to block TLR9-mediated IFNα production, but whether BDCA2 plays a role in that as well is not known. Interestingly, Takahashi et al¹⁶⁵ have provided evidence that pDCs that infiltrate the liver during HCV infection could be a major source of type I IFNs. In these studies, co-cultivation of pDCs with HCV-infected hepatocytes resulted in marked IFN production in proportion to the number of HCV-infected cells. IFN production was mediated by TLR7, and not TLR9, a finding consistent with earlier studies reporting that HCV inhibits TLR9 but not the TLR7-mediated pathway to suppress IFN production.^{79, 80, 164} This essentially helps explain why infection with HCV leads to a robust expression of IFN-stimulated genes in liver^166,167 despite its remarkable ability to attenuate IFN production by infected hepatocytes.¹⁶⁸

Recent studies have shown that persistent viruses can induce the activity of immunosuppressive enzymes in DCs, which leads to suppression of antiviral T-cell response. Tryptophan-catabolizing indoleamine 2,3 dioxygenase (IDO) activity seems to play a central role in the suppressive function of DCs.¹⁶⁹ On direct exposure to HIV-1, DCs induce IDO activity, which leads to inhibition of CD4⁺ T-cell proliferation in vitro.¹⁷⁰ Additionally, HIV-1-induced IDO activity in pDCs leads to differentiation of naive T cells into CD4⁺CD25⁺FOXP3⁺ regulatory T cells with suppressive function.¹⁷¹ In simian immunodeficiency virus-infected macaques, IDO activity peaked at the same time as the increase in plasma viremia, as well as expansion of the CD4⁺CD25⁺FOXP3⁺ T-cell subset, which may play an important role in curbing the SIV-specific CD4⁺ T-cell response.¹⁷² Enhanced IDO activity is found in both HIV-1 and HCV-infected patients; further investigation is thus needed to completely understand its role in the regulation of the cellular immune response against these viruses.

The inability of DCs to facilitate the clearance of HIV-1 and HCV-infection patients leads to chronic immune activation. Systemic chronic immune activation is already believed to be the primary driver of HIV-1 disease progression and the focus is now on understanding its role in the development of liver fibrosis, cirrhosis, or hepatocellular carcinoma in HCV-infected patients. Recent reports have shown that chronic pDC stimulation and IFNα production in HIV-1-infected individuals are associated with higher risk of progression to AIDS. It is thus becoming increasingly important to understand the role of DCs in HIV-1 and HCV-mediated diseases.

Crosstalk between DCs and NK Cells

In addition to their direct antiviral functions, NK cells are capable of regulating antiviral immunity by modulating the function of DCs.^{173, 179} Crosstalk between DCs and NK cells promotes activation of both cell types. Activated DCs upregulate NK cell effector functions and NK cells, in turn, induce further maturation of DCs. Fernandez et al¹⁷³ showed that DCs are able to promote anti-tumor activity of NK cells activity in vivo. Since then, many studies have investigated the role of DCs in the “priming” of NK cells,^180,181 a process that involves both cell-cell interactions and cytokine production. Cytokines produced by mDCs, such as IL-12 and IL-18, can promote NK cell production of IFNγ in vitro.^{175,177,180,181} Moreover, pDC production of type I IFNs and cell-cell contact is essential for promoting NK cell proliferation and cytotoxicity.^{173,174,176,177} IFNγ produced by activated NK cells promotes T_H1 cell polarization.^174,178 NK cell-mediated activation of DCs is also known to promote the differentiation of DCs that are more efficient at inducing CTL responses.¹⁷⁹ Furthermore, DC uptake of apoptotic bodies produced as a result of NK cell-mediated lysis of virus-infected cells can promote DC maturation and presentation of viral antigens to T cells. Therefore, in addition to their direct cytotoxic effects, NK cells are capable of boosting the adaptive immune response.

In a process referred to as “DC editing,” NK cells can kill immature DCs.¹⁸¹ In vitro studies have demonstrated that a low ratio of NK cells to immature DCs promotes DC maturation, whereas a higher ratio of NK cells to immature DCs can result in NK cell-mediated killing of DCs.¹⁷⁹ NKp30 on NK cells plays an important role in this process.¹⁸¹ It is clear that the crosstalk between DCs and NK cells plays an important role in regulating the antiviral immune response. In the next section we discuss the impact of HIV-1 and HCV on this crosstalk.

HIV-1

Recent evidence has suggested that the crosstalk between DCs and NK cells is disrupted during HIV-1 infection. mDCs from HIV-1-infected individuals show reduced secretion of IL-12, IL-15, and IL-18, resulting in decreased NK cell activation. During HIV-1 infection, activation of NK cells by pDCs is impaired because of their lower responsiveness to type I IFNs.¹⁸² The ability of NK cells to kill immature DCs is reduced in individuals with chronic HIV-1 infection.¹⁸³ This defect in NK cell-mediated DC editing appears to be largely the result of an increase in the percentage of CD56^– NK cells with impaired NKp30 function.¹⁸⁴ The mechanism of HIV-1-mediated impairment of DC-NK cell crosstalk is not fully understood. The effects of two HIV-1 proteins, Tat and Nef, on DCs and NK cells have been described.^185,186 HIV-1-infected DCs have an upregulation of cell death inhibitors that protects them from TRAIL (tumor necrosis factor-related apoptosis-inducing ligand)-mediated NK cell cytotoxicity. This upregulation of cell death inhibitors is mediated by the high-mobility group box 1 protein (HMGB1).¹⁸⁷ Furthermore, the crosstalk of HIV-1- infected DCs with NK cells has been shown to promote viral replication in HIV-1-infected DCs; however, this can be prevented by blocking HMGB1 activity.¹⁸⁸ In addition, increased production of IL-10 during HIV-1 infection limits NK cell-mediated lysis of immature DCs, which results in accumulation of partially mature, poorly immunogenic DCs in the lymph nodes of infected individuals.¹⁸⁹

HCV

Compared to healthy individuals^{190, 194} and spontaneous resolvers of HCV infection,^{192, 195, 197} the frequency of NK cells in peripheral blood is reduced in individuals with chronic HCV infection. Additionally, individuals with chronic HCV infection have an increase in NK cell frequency following successful IFN/RBV therapy. IL-15 is a cytokine that plays a pivotal role in NK cell development, proliferation, and function, and therefore reduction in NK cell frequency could be attributed to reduction in IL-15 levels. In this regard, Meier et al have shown a significant reduction in IL-15 levels in HCV patients when compared to healthy controls; they have also shown that exogenous IL-15 is able to rescue the NK cells of HCV-infected patients from apoptosis, resulting in their increased ex vivo proliferation and function.¹⁹³ DCs from HCV-infected individuals are deficient in IL-15 production upon stimulation with IFNα¹⁹⁸ and a consequence of this DC dysfunction could be inadequate development and proliferation of NK cells. DCs express MHC class I-related chain A and B (MICA/B), which are ligands for NK cell activating receptor NKG2D. Interestingly, IL-15 is known to induce the expression of MICA/B on DCs; therefore, reduced production of IL-15 during chronic infection with HCV can affect DC activation of NK cells.¹⁹⁸

Human liver epithelial cells express HLA-E, a ligand for CD94/NKG2A expressed on NK cells. In comparison to healthy individuals, NK cells from individuals with chronic HCV infection show higher expression of CD94/NKG2A and produce IL-10 and transforming growth factor-β (TGFβ) when cultured with human liver epithelial cells, most of which express HLA-E. IL-10 and TGFβ production is known to correlate with impaired activation of DCs. A blockade of NKG2A has been demonstrated to restore the ability of NK cells (from HCV-infected individuals) to activate DCs. The blockade also stimulates NK cells to generate T_H 1 - polarized CD4⁺ T cells. It is important to realize, however, that HLA-E may also be expressed on cells other than liver epithelial cells. In fact, HCV is known to stabilize HLA-E expression on intrahepatic APCs;¹⁹⁹ this represents a mechanism by which HCV modulates the NK cell response. The dysregulation of DC-NK cell crosstalk might also have significant consequences for the antiviral T-cell and B-cell responses. The development of therapeutic interventions aimed at enhancing the immune response against HIV-1 and HCV will require a complete understanding of the molecular mechanisms involved in DC-NK cell crosstalk and how it becomes disrupted during chronic HIV-1 and HCV infection.

Modulation of the Immunological Synapse: Role in HIV-1 and HCV Pathogenesis

The generation of specific immune responses against a pathogen requires the interaction between T cells (expressing the cognate receptor) and antigen-loaded mature DCs in the lymph nodes.^1,200,201 During this process a specialized cell-cell junction called the immunological synapse (IS) is formed between these two cell types.^200–206 Modulation of IS by HIV-1 (Fig. 3) has been identified as one of the important strategies used by HIV-1 to evade the host immune response in order to spread rapidly within the host.

Figure 3.

Modulation of immunological synapse by HIV-1 and HCV.

HIV-1

The degree of viral replication in CD4⁺ T cells depends on their state of activation. In vivo studies have shown that HIV-1 and SIV¹⁷² can replicate in T cells that have a low activation profile, albeit viral replication is much more efficient in activated T cells.^207–210 A lack of T-cell activation has been shown to block several steps in the HIV-1 life cycle, including reverse transcription, nuclear import, and integration of the viral genome, as well as transcription and export of multiply spliced viral mRNA after its entry into quiescent CD4⁺ T cells.^90,211–214 Conversely, T-cell activation through T-cell receptor (TCR) ligation or other stimuli often initiates homeostatic programs of apoptosis such as activation-induced cell death (AICD).^215,216 The rapid death of infected cells will limit viral production and therefore it is postulated that the virus modulates IS to establish a balance between an apoptosis-prone activation state and the replication-unfavorable environment of resting T cells.²¹⁷ HIV-1 protein Nef has been shown to lower the threshold of TCR activation, resulting in induction of an intermediate activation state that prevents AICD and at the same time allows for efficient HIV-1 replication.^218–222 This model is also supported by the “bystander effect” hypothesis, which proposes that most of the apoptotic cell death occurring in HIV-1 infection involves uninfected cells rather than infected cells. In addition to facilitating efficient viral replication, infected lymphocytes are also able to efficiently transfer HIV-1 to uninfected lymphocytes through the formation of a virological synapse (Fig. 3). Contrary to what we have discussed above, several groups have shown that various HIV-1 proteins induce apoptosis of infected CD4⁺ T cells. This could be due to the fact that the actual in vivo concentrations of these proteins seen in HIV-1 infection are largely unknown and in vitro experiments involving overexpression of a particular protein may not be reflective of its in vivo effects. Another interesting point is that many HIV-1 proteins such as Nef and Vpr have been shown to possess both proapoptotic and antiapoptotic effects depending on their expression levels, the activation state of infected T cells, and many other factors.

Several studies have shown that impairment of IS formation between infected lymphocytes and APCs is Nef-dependent.^220,223,224 Rabi et al²²⁵ have shown that unstimulated primary CD4⁺ T cells from HIV-1-positive “elite controllers”—plasma HIV-RNA values persistently below 50 copies/mL throughout the course of infection—are as susceptible to HIV-1 entry and productive infection as viremic patients, suggesting that differences in HIV-1 entry and infection of CD4⁺ T cells alone cannot explain the elite control of viral replication. It is also known that people who control HIV-1 often have CD4⁺ T cells that express high amounts of IL-2 and IFNγ in response to HIV peptides.²²⁶ This implies that infected CD4⁺ T cells can play an important role in controlling the infection and that in addition to ensuring that the HIV-1-infected T cells do not limit viral production by undergoing AICD, impairment of IS by HIV-1 can prevent them from participating in successful clearance of the virus.

Most of the studies about IS have centered on the T-cell side of the IS (IS-T), whereas the functional significance of the DC side (IS-DC) is poorly understood. It is known that DCs from HIV-1-infected patients show increased apoptosis compared to uninfected controls.^{227, 229} It has been shown that the stable formation of IS results in activation of kinase Akt1. Activation of Akt1 promotes the localization of prosurvival transcription factor NF-κB into the nucleus and proapoptotic transcription factor FOXO1 out of nucleus into the cytoplasm.²³⁰ Therefore, it can be hypothesized that HIV-1-mediated disruption of IS initiates a signaling cascade that results in DC apoptosis. Some surface receptors located at the IS-DC, including ICAM-2,²³¹ CD22,²³² and CD40,²³⁰ lead to the activation of Akt1 in DCs. Among these receptors, CD40 is particularly interesting as in addition to inducing the activation of Akt1 in DCs,²³⁰ CD40 has been shown to extend their survival.²³³ CD40 stimulation results in an increased abundance both of the antiapoptotic Bcl-2 member Bcl-X_L and of the cellular inhibitor of apoptosis protein 2 (cIAP-2).²³⁴ This suggests that CD40 might play an important role in the activation of Akt1 and the antiapoptotic signaling relayed from IS-DC.²³⁰ This suggestion is supported by studies in CD40-deficient mice and CD40L-deficient mice that do not elicit CD4⁺ and CD8⁺ T-cell-dependent immunity, underscoring the importance of CD40 ligation in prosurvival effects of IS, as well as generation of adaptive immune response. Besides Akt1, Notch has also been implicated in inhibiting the apoptosis of DCs by inducing the activation of STAT3 (signal transducer and activator of transcription 3), a transcription factor known to promote cell survival. Several studies have reported DC-induced apoptosis of T cells.^235–240 Because DCs are known to be susceptible to HIV-1 infection, it will be interesting to study whether disruption of IS-DC by HIV-1 is responsible for triggering DC-induced apoptosis of uninfected T cells during IS formation. It will also help to shed light on the role of DCs on bystander T-cell death during HIV-1 infection.

One of the studies has shown that cytoskeletal remodeling mediated by Wiskott-Aldrich syndrome protein (WASp) in DCs is necessary for normal immune synapse formation and T-cell priming.²⁴¹ In DCs, the loss-of-function mutation of WASp can also abolish the activation of NK cells by DCs.²⁴² The HIV-1 pathogenicity factor Nef is known to modulate WASp activity, leading to altered TCR signaling in T cells;²⁴³ in contrast, the effect of HIV-1 on WASp within DCs is not well understood. HIV-1 protein Nef has been shown to trigger the secretion of various cytokines and chemokines (including CC-chemokine ligand 3 [CCL3] and CCL4) by infected APCs.^244–247 This can lead to increased HIV-1 replication in CD4⁺ T cells that get attracted to APCs in response to CCL3 and CCL4 secretion.²⁴⁴

HCV

As discussed in previous sections of this study, while HCV is primarily a non-lymphotropic virus, it has also been found to replicate in PBMCs as well. Although the impact of HCV on IS has not been investigated thoroughly, we hypothesize that HCV can modulate IS either by infecting DCs and/or T cells or via soluble HCV proteins. Modulation of IS can interfere with T-cell activation, leading to weak T-cell response; additionally, suboptimal activation of T cells can prevent AICD, thus allowing HCV to persist inside them for longer periods. Like HIV-1, HCV could also exploit IS to spread efficiently across PBMCs and this may explain why neutralizing-antibodies against HCV do not always clear the virus.

A widely used approach to assess the antigen-presenting function of DCs is their ability to induce proliferation of allogeneic naïve T cells. Many studies have demonstrated that this function is impaired in MDDCs from patients with HCV infection.^153,158 DCs expressing HCV core and E1 proteins have been shown to prime CD4⁺ T cells abnormally.²⁴⁸ HCV core protein impairs the priming of specific T-cell responses by DCs even when it is added exogenously in the culture media.²⁴⁹ This is an important observation because HCV core protein is present in the sera of infected patients and could therefore be responsible for mediating a number of T-cell-inhibitory effects in vitro and in vivo. Krishnadas et al²⁵⁰ studied the effect of soluble HCV proteins on DCs of healthy uninfected individuals and showed that individual HCV proteins (core, NS3, NS4, NS5) or fused polyprotein (core-NS3-NS4) can impair functions of both immature and mature DCs by downregulating the expression of co-stimulatory and antigen presentation molecules, reducing IL-12 secretion, inducing the expression of Fas ligand (FasL) to mediate apoptosis, interfering with allostimulatory capacity, and inhibiting TLR signaling and nuclear translocation of NF-κB. Interestingly, HCV proteins did not directly inhibit T-cell proliferation, suggesting that they might instead affect the ability of DCs to conjugate with T cells during IS formation. Modulation of IS by both HIV-1 and HCV can have profound effects on the rate of viral replication as well as generation of adaptive immune response. The impairment of IS by these two viruses, especially through their interaction with DCs is gaining a lot of interest. In years to come, we will notice a significant growth in our understanding of IS-DC and how various chronic viruses affect it.

Immune Response in the Liver: Role of Hepatic Antigen Presenting Cells

Besides liver-resident DCs, several other liver cell populations such as LSECs, stellate cells, and Kupffer cells²⁵¹ can present antigens and influence the antiviral immune response. However, these APCs exist in a state of active tolerance, thus contributing towards a tolerogenic liver environment, as evidenced by spontaneous acceptance of liver allografts.²⁵² These liver APCs continuously secrete immunosuppressive cytokines such as IL-10 and TGFβ1.²⁵³ This raises the question of whether the tolerogenic properties of liver APCs contribute towards the establishment of persistent HCV infection and whether liver is a site favoring the evasion of immune response against HCV, as well as other viruses.

Access to liver biopsies from HCV-infected and HIV-1/HCV co-infected patients is limited; isolation of adequate numbers of hepatic APCs is also difficult. Therefore, little is known about the role of hepatic DCs in HCV infection. Kupffer cells and LSECs do not support HCV replication. In vivo studies have demonstrated that hepatic DCs and LSECs can present exogenous antigen to naïve T cells, but this does not lead to effective T-cell response, either due to inhibition of T-cell polyfunctionality or due to acquisition of an immunosuppressive phenotype by T cells. Uptake of viral particles by hepatic APCs may prime CD4⁺CD25⁺FOXP3⁺ regulatory T cells, which are known to dampen the CD8⁺ T-cell response. This results in failure of the immune system to eradicate the virus from the liver. In chronic HCV infection, antigen-specific CD8⁺ T cells in liver are frequently reported to become dysfunctional and unable to secrete IFNγ and IL-2.²⁵⁴ In light of these observations, it is important to advance our understanding of the role of hepatic APCs in priming of HCV-specific T cells.

The antigen presentation ability of hepatocytes has not been studied thoroughly since hepatocytes are generally inaccessible to naive T cells as a result of the barrier formed by LSECs. However, electron microscopy studies have shown that hepatocytes contain microvilli that can pass through fenestrations in the endothelium, allowing them to make contact with the naive T cells in the sinusoidal lumen.²⁵⁵ Normally, hepatocytes do not express MHC class II molecules, but aberrant expression of MHC class II molecules has been noted in cases of clinical hepatitis.^256,257 Therefore, it will not be unreasonable to believe that hepatocytes can induce HCV-specific CD4⁺ T cells or modulate the antiviral activity of pre-activated CD4⁺ T cells. Studies on transgenic mice have also shown that hepatocytes can directly stimulate CD8⁺ T cells, although the stimulated T cells seem to lack cytotoxicity, possibly due to an absence of co-stimulatory molecules on hepatocytes.^258,259

Impact of Host Genetic Variations on DC Functions during HIV-1 and HCV Infection

Studying the role of host genetic variations in determining infection outcome will facilitate our understanding of HIV-1 and HCV pathogenesis. Several genetic polymorphisms have been reported to be associated with low rates of spontaneous clearance, poor treatment response, or accelerated disease progression during the chronic phase of infection. Some of these polymorphisms or rare mutations are found in genes that control DC functions such as recognition of virus, priming of T cells, migration to lymph nodes, and cross talk with NK cells (summarized in Table 2). Understanding the mechanistic underpinnings behind these genetic associations will allow us to gain a deeper insight into the immune evasion strategies adopted by HIV-1 and HCV infection, in addition to helping us devise better treatment options.

Table 2.

Impact of host genetic variations on DC functions during HIV-1 and HCV infection.

DC function affected by the polymorphism	Virus	Gene involved	References
Early recognition of viral signatures and induction of innate and adaptive immune responses	HCV	TLR2	261
		TLR3	262,263
		TLR7	264–267
		TLR8	267
		IRF1	268
		IRF7	269
	HIV	TLR3	270
		TLR4	271
		TLR7	272,273
		TLR8	274
		TLR9	271,275–277
		IRF1	278
		IRF7	279
Presentation of viral peptides to T cells as well as crosstalk with NK cells	HCV	HLA class II	172,280–304
	HIV	HLA class II	305–308
Binding to viral envelope, interaction with naïve T cells and migration	HCV	DC-SIGN	309
	HIV	DC-SIGN	310–313

Future of Anti-HCV Treatment with and without HIV-1 Co-Infection

Since its introduction in 1996, highly active antiretroviral treatment (HAART) against HIV-1 has been quite successful in controlling HIV-1 infection. The current standard treatment for treating HCV genotype 2–3 infection is a combination of pegylated interferon (PEG-IFN) and an antiviral drug, ribavirin (RBV). Current therapy for HCV genotype 1 consists of an HCV protease inhibitor, telaprevir or boceprevir, in combination with PEG-IFN and RBV. In contrast to HIV-1, treatment of HCV has been difficult because of the low rate of success and a high rate of treatment discontinuation, primarily owing to side effects of IFN/RBV therapy. A sustained virological response is defined as persistent absence of serum HCV RNA for 6 months or longer after therapy and is generally regarded as a cure for HCV infection. However, HCV treatment is toxic and has significant side effects such as anemia, thrombocytopenia, neutropenia, diarrhea, and flulike symptoms such as fever, chills, fatigue, headache, and muscle aches. Therefore, it becomes very important to determine the predictive factors of successful treatment response.

In order to understand the role of DCs in treatment outcome—as well as to study the impact of IFN/RBV therapy on DCs—various studies have attempted to characterize the phenotypic and functional status of blood DCs before or during IFN/RBV therapy. Table 3 highlights those studies that have demonstrated a correlation between the phenotypic and/or functional status of DCs with sustained virological response. Both IFN and RBV have nonspecific and largely unknown mechanisms of action; therefore, various drugs that can directly target HCV at various stages of replication are currently under development (summarized in Table 4). Supplementation of PEG-IFN/RBV with telaprevir or boceprevir in a treatment-naive population improved sustained a virological response of between 40% and 75%. Additionally, treatment duration was shortened from 48 weeks to 24–48 weeks for approximately 50% of patients. In treatment-experienced populations, the treatment response after supplementing PEG-IFN/RBV with telaprevir or boceprevir was ~30% for non-responders, ~55% for partial responders, and 75% to 85% for relapsers. Telaprevir and boceprevir and many other drugs that are in the pipeline will begin a new era of HCV treatment, the ultimate goals of which will be to shorten the duration of therapy, improve sustained virological response rates, and minimize the side effects. Many clinical trials are underway which will address whether these direct-acting antiviral (DAA) drugs will be equally efficacious during HIV-1/HCV co-infection. Moreover, in light of the suggested role of DCs in harboring and disseminating HCV, it will be interesting to study if the efficacy of anti-HCV drugs is dependent on their ability to clear the virus from DCs.

Table 3.

DC-related predictors of sustained virological response to the IFN/RBV therapy.

Treatment time point	Predictor of sustained virological response	Ref.
Baseline^a	High CD83 expression and low IL-10 production of DCs	4,314
Week 4^b and Week 48^b	Higher allostimulatory activity of MDDCs from patients	5,315
Post-treatment^c	Higher percentage of BDCA-1⁺ mDCs, as well as higher levels of CD86⁺ cells, in both BDCA-1⁺ mDCs and pDCs	6,316
	CD86 and CD83 increase as well as ERK1/2 or p38-MAPK phosphorylation upon TLR7-cell triggering in MDDCs
Baseline^d	Lower chemotaxis index of pDCs to CXCL12 and CXCL10	7,161
Week 12^e	Higher frequency of pDCs	8,317

Notes:

Weekly administration of PEG-IFNα2b (1.5 μg/kg of body weight) by subcutaneous injection (s.c.) plus oral ribavirin at a dose of 1000–1200 mg, depending on the body weight, for 24 weeks;

PEG-IFNα2b (75–135 μg/week, s.c.) plus oral ribavirin (600–1000 mg/day) for 48 weeks;

PEG-IFNα2b (1.5 μg/kg of body weight/week, s.c.) plus oral ribavirin (800–1200 mg/day) for 6 or 12 months according to the HCV genotype;

PEG-IFNα-2a (180 μg/week, s.c.) plus oral ribavirin (1000–1200 mg/day) for up to 48 weeks;

PEG-IFNα2b (75–135 μg/week, s.c.) plus oral ribavirin (600–1000 mg/day) for 48 weeks.

Table 4.

Direct-acting antiviral agents for hepatitis C virus infection.

HCV protein	Function	Inhibitors
HCV protein	Function	Phase I	Phase II	Phase III	Licensed
NS3/NS4A protease	Post-translational processing of HCV poly-protein	GSK2336805 IDX320 MK-5172 VX-985	ACH-0141625 BMS-650032 GS-9256 GS-9451 ABT-450/r^a	TMC435 BI 201335	Telaprevir Boceprevir
NS5B polymerase	RNA-dependent RNA polymerase required for copying the HCV-RNA genome as well as mRNA synthesis	Nucleos(t)ide analogues GS-6620	Nucleos(t)ide analogues IDX184 PSI-7977 Mericitabine INX-08189	None	None
		Non-nucleos(t)ide analogues GS-9669	Non-nucleos(t)ide analogues ABT-333 ABT-072 GS-9190 VX-222 VCH-916	None	None
NS5A	Involved in HCV replication but the exact function is not clear	AZD7295 PPI-461	ABT-267 GS-5885	BMS-790052	None

Note: Latest update on these drugs is available at: http://clinicaltrials.gov/.

Conclusions and Future Perspectives

In the last few years, enough evidence has accumulated to suggest that both HIV-1 and HCV target DCs to cripple the innate and adaptive immune response directed against them. Both viruses affect the ability of mDCs to produce key cytokines that are necessary for the development and activation of an effective T-cell response. In addition, they seem to use similar strategies to attenuate the potent antiviral IFNα response in pDCs. Besides interfering with the natural antiviral activity of DCs, these viruses also use DCs as vehicles for widespread dissemination within the host.

In future, the key issues for improving our understanding of the interaction of HIV-1 and HCV with DCs include the molecular mechanisms of viral entry, processing, and presentation by DCs; the identification of mechanisms that regulate the balance between intrahepatic tolerance and immunity; the impact of HCV, if any, on the formation of immunological synapse between DCs and T cells; molecular mechanisms involved in DC-NK cell cross-talk; and the role of HCV-infected DCs in aiding viral transmission. Answers to these questions will not only help us understand the immunobiology of these two viruses but will also contribute towards the development of better treatment strategies aimed at generating a protective immune response that controls viral infection, without any significant side effects.

Author Contributions

Wrote the first draft of the manuscript: MS, PJ. Contributed to the writing of the manuscript: MS, PJ, ZKK. Agree with manuscript results and conclusions: MS, AHT, ZKK, PJ. Jointly developed the structure and arguments for the paper: MS, PJ. Made critical revisions and approved final version: MS, AHT, ZKK, PJ. All authors reviewed and approved of the final manuscript.

Funding

We wish to acknowledge United States Public Health Service/National Institutes of Health Grants R01 AI077414-01 (to P J) and AI093172 (to Z K) and internal funds from the Department of Microbiology and Immunology, Drexel University College of Medicine to PJ.

Competing Interests

Author(s) disclose no potential conflicts of interest.

Disclosures and Ethics

As a requirement of publication author(s) have provided to the publisher signed confirmation of compliance with legal and ethical obligations including but not limited to the following: authorship and contributorship, conflicts of interest, privacy and confidentiality and (where applicable) protection of human and animal research subjects. The authors have read and confirmed their agreement with the ICMJE authorship and conflict of interest criteria. The authors have also confirmed that this article is unique and not under consideration or published in any other publication, and that they have permission from rights holders to reproduce any copyrighted material. Any disclosures are made in this section. The external blind peer reviewers report no conflicts of interest.

Footnotes

Abbreviations

References

Banchereau

, Steinman

R.M.

Dendritic cells and the control of immunity. Nature. 1998; 392: 245–52.

Kawai

, Akira

The roles of TLRs, RLRs and NLRs in pathogen recognition. Int Immunol. 2009; 21(4): 317–37.

Trombetta

E.S.

, Mellman

Cell Biology of antigen processing in vitro and in vivo. Annu Rev Immunol. 2005; 23(1): 975–1028.

Banchereau

Immunobiology of dendritic cells. Annu Rev Immunol. 2000; 18: 767–811.

, Liu

Y.J.

Development of dendritic-cell lineages. Immunity. 2007; 26: 741–50.

Steinman

R.M.

, Haemmi

Dendritic cells: translating innate to adaptive immunity. Curr Top Microbiol Immunol. 2006; 311: 17–58.

Romagnani

Activation of human NK cells by plasmacytoid dendritic cells and its modulation by CD4+ T helper cells and CD4+CD25hi T regulatory cells. Eur J Immunol. 2005; 35: 2452–8.

Liu

Y.J.

IPC: professional type 1 interferon-producing cells and plasmacytoid dendritic cell precursors. Annu Rev Immunol. 2005; 23: 275–306.

Colonna

, Trinchieri

, Liu

Y.J.

Plasmacytoid dendritic cells in immunity. Nature Immunol. 2004; 5: 1219–26.

10.

Tel

, Lambeck

A.J.A.

, Cruz

L.J.

, Tacken

P.J.

, de Vries

I.J.M.

, Figdor

C.G.

Human Plasmacytoid dendritic cells phagocytose, process, and present exogenous particulate antigen. J Immunol. 2010; 184(8): 4276–83.

11.

Villadangos

J.A.

, Young

Antigen-presentation properties of plasmacytoid dendritic cells. Immunity. 2008; 29(3): 352–61.

12.

West

A.P.

, Koblansky

A.A.

, Ghosh

Recognition and signaling by toll-like receptors. Annu Rev Cell Dev Biol. 2006; 22(1): 409–37.

13.

Cervantes-Barragan

, Lewis

K.L.

, Firner

Plasmacytoid dendritic cells control T-cell response to chronic viral infection. Proc Natl Acad Sci U S A. 2012; 109(8): 3012–7.

14.

Smit

J.J.

The balance between plasmacytoid DC versus conventional DC determines pulmonary immunity to virus infections. PLoS One. 2008; 3: e1720.

15.

GeurtsvanKessel

C.H.

Clearance of influenza virus from the lung depends on migratory langerin+CD11b- but not plasmacytoid dendritic cells. J Exp Med. 2008; 205: 1621–34.

16.

Jain

, Ahuja

, Khan

Z.K.

Modulation of dendritic cell maturation and function by the Tax protein of human T cell leukemia virus type 1. J Leukoc Biol. 2007; 82(1): 44–56.

17.

Jain

, Manuel

S.L.

, Khan

Z.K.

, Ahuja

, Quann

, Wigdahl

DC-SIGN mediates cell-free infection and transmission of human T-cell lymphotropic virus type 1 by dendritic cells. J Virol. 2009; 83(21): 10908–21.

18.

Ahuja

, Kampani

, Datta

, Wigdahl

, Flaig

K.E.

, Jain

Use of human antigen presenting cell gene array profiling to examine the effect of human T-cell leukemia virus type 1 Tax on primary human dendritic cells. J Neurovirol. 2006; 12(1): 47–59.

19.

Ahuja

, Lepoutre

, Wigdahl

, Khan

Z.K.

, Jain

Induction of pro-inflammatory cytokines by human T-cell leukemia virus type-1 Tax protein as determined by multiplexed cytokine protein array analyses of human dendritic cells. Biomed Pharmacother. 2007; 61(4): 201–8.

20.

Rahman

, Khan

Z.K.

, Jain

The Tug-of-war between dendritic cells and human chronic viruses. Int Rev Immunol. 2011; 30(5-6): 341–65.

21.

Rahman

, Khan

Z.K.

, Wigdahl

, Jennings

S.R.

, Tangy

, Jain

Murine FLT3 ligand-derived dendritic cell-mediated early immune responses are critical to controlling cell-free human T cell leukemia virus type 1 infection. J Immunol. 2011; 186(1): 390–402.

22.

Rahman

, Manuel

S.L.

, Khan

Z.K.

Depletion of dendritic cells enhances susceptibility to cell-free infection of human T cell leukemia virus type 1 in CD11c-diphtheria toxin receptor transgenic mice. J Immunol. 2010; 184(10): 5553–61.

23.

Manuel

S.L.

, Schell

T.D.

, Acheampong

, Rahman

, Khan

Z.K.

, Jain

Presentation of human T cell leukemia virus type 1 (HTLV-1) Tax protein by dendritic cells: the underlying mechanism of HTLV-1-associated neuroinflammatory disease. J Leukoc Biol. 2009; 86(5): 1205–16.

24.

Mostoller

, Norbury

, Jain

, Wigdahl

Human T-cell leukemia virus type I Tax induces the expression of dendritic cell markers associated with maturation and activation. J Neurovirol. 2004; 10(6): 358–71.

25.

Grant

, Jain

, Nonnemacher

AP-1-directed human T cell leukemia virus type 1 viral gene expression during monocytic differentiation. J Leukoc Biol. 2006; 80(3): 640–50.

26.

Jain

, Mehta

, Nickens

, Philip

, Shetty

, Sinnathamby

Investigation of plasma biomarkers in HIV-1/HCV mono- and coinfected individuals by multiplex iTRAQ quantitative proteomics. OMICS. 2011; 15(10): 705–17.

27.

Tran

, El Baz

, Cuconati

, Arthos

, Jain

, Khan

Z.K.

A novel high throughput screening assay to identify inhibitor of HIV-1 gp120 interaction with DC-SIGN. J Antivir Antiretrovir. 2011; 3: 49–54.

28.

Boukli

, Shetty

, Cubano

Unique and differential protein signatures for HIV-1 and HCV mono-infection versus co-infection. Clin Proteomics. Sep 7 2012; 9(1): 11. [Epub ahead of print.]

29.

Rehermann

, Nascimbeni

Immunology of hepatitis B virus and hepatitis C virus infection. Nature Rev Immunol. 2005; 5: 215–29.

30.

Guidotti

L.G.

, Chisari

F.V.

Immunobiology and pathogenesis of viral hepatitis. Annu Rev Pathol. 2006; 1: 23–61.

31.

Gandhi

R.T.

, Walker

B.D.

Immunologic control of HIV-1. Annu Rev Med. 2002; 53: 149–72.

32.

McMichael

A.J.

, Rowland-Jones

S.L.

Cellular immune responses to HIV. Nature. 2001; 410: 980–7.

33.

Nattermann

, Vogel

, Nischalke

H.D.

The transforming growth factor-[beta] high-producer genotype is associated with response to hepatitis C virus-specific therapy in HIV-positive patients with acute hepatitis C. AIDS. 2008; 22(11): 1287–92, 1210.1097/QAD.1280b1013e3282f1285daa.

34.

Simon

, Ho

D.D.

, Abdool Karim

HIV/AIDS epidemiology, pathogenesis, prevention, and treatment. Lancet. 2006; 368: 489–504.

35.

UNAIDS. 2009 AIDS Epidemic update. Geneva, Switzerland. 2009. Available at: http://www.unaids.org/en/dataanalysis/epidemiology/2009aidsepidemicupdate/. Accessed on Nov 2, 2011.

36.

HIV/AIDS in the United States. CDC HIV/AIDS facts, 2009. Available at: http://www.cdc.gov/hiv/topics/surveillance/basic.htm. Accessed on Nov 2, 2011.

37.

Prejean

, Song

, Hernandez

Estimated HIV incidence in the United States, 2006–2009. PLoS One. 2011; 6(8): e17502.

38.

Williams

Global challenges in liver disease. Hepatology. 2006; 44: 521–6.

39.

World Health Organization factsheet on Hepatitis C, Jun 2011. Available at: http://www.who.int/mediacentre/factsheets/fs164/en/.

40.

Sherman

K.E.

, Rouster

S.D.

, Chung

R.T.

, Rajicic

Hepatitis C virus prevalence among patients infected with human immunodeficiency virus: a cross-sectional analysis of the US adult AIDS clinical trials group. Clinical Infectious Diseases. 2002; 34(6): 831–7.

41.

Alter

M.J.

Epidemiology of viral hepatitis and HIV co-infection. J Hepatol. 2006; 44: S6–9.

42.

Sulkowski

M.S.

, Thomas

D.L.

Hepatitis C in the HIV-Infected Person. Ann Intern Med. 2003; 138(3): 197–207.

43.

Bauer

, Tampe

Herpes viral proteins blocking the transporter associated with antigen processing TAP—from genes to function and structure. Curr Top Microbiol Immunol. 2002; 269: 87–99.

44.

Jason

T.B.

, Smeaton

, Hiasa

Detection of hepatitis C virus (HCV) in serum and peripheral-blood mononuclear cells from HCV-monoinfected and HIV/HCV-coinfected persons. J Infect Dis. 2005; 192(2): 258–65.

45.

Kaiser

, Niederost

, Joos

Equal amounts of intracellular and virion-enclosed hepatitis C virus RNA are associated with peripheral-blood mononuclear cells in vivo. J Infect Dis. 2006; 194(12): 1713–23.

46.

Pal

, Sullivan

D.G.

, Kim

Productive replication of hepatitis C virus in perihepatic lymph nodes in vivo: implications of HCV lymphotropism. Gastroenterology. 2006; 130(4): 1107–16.

47.

Laskus

, Operskalski

E.A.

, Radkowski

Negative-strand hepatitis C virus (HCV) RNA in peripheral blood mononuclear cells from anti-HCV-positive/HIV-infected women. J Infect Dis. 2007; 195(1): 124–33.

48.

Pham

T.N.

, King

, Macparland

S.A.

Hepatitis C virus replicates in the same immune cell subsets in chronic hepatitis C and occult infection. Gastroenterology. 2008; 134(3): 812–22.

49.

Kawamura

R5 HIV productively infects Langerhans cells, and infection levels are regulated by compound CCR5 polymorphisms. Proc Natl Acad Sci U S A. 2003; 100: 8401–6.

50.

Zaitseva

Expression and function of CCR5 and CXCR4 on human Langerhans cells and macrophages: implications for HIV primary infection. Nature Med. 1997; 3: 1369–75.

51.

Niedecken

, Lutz

, Bauer

, Kreysel

H.W.

Langerhans cell as primary target and vehicle for transmission of HIV. The Lancet. 1987; 330(8557): 519–20.

52.

Berger

Isolation of human immunodeficiency virus type 1 from human epidermis: virus replication and transmission studies. J Invest Dermatol. 1992; 99: 271–7.

53.

Soto-Ramirez

L.E.

HIV-1 Langerhans’ cell tropism associated with heterosexual transmission of HIV. Science. 1996; 271: 1291–3.

54.

Ludewig

, Gelderblom

H.R.

, Becker

, Schafer

, Pauli

Transmission of HIV-1 from productively infected mature Langerhans cells to primary CD4+ T lymphocytes results in altered T cell responses with enhanced production of IFN-[gamma] and IL-10. Virology. 1996; 215: 51–60.

55.

Blauvelt

Productive infection of dendritic cells by HIV-1 and their ability to capture virus are mediated through separate pathways. J Clin Invest. 1997; 100: 2043–53.

56.

Granelli-Piperno

, Delgado

, Finkel

, Paxton

, Steinman

R.M.

Immature dendritic cells selectively replicate macrophagetropic (M-tropic) human immunodeficiency virus type 1, while mature cells efficiently transmit both M- and T-tropic virus to T cells. J Virol. 1998; 72: 2733–7.

57.

Granelli-Piperno

, Finkel

, Delgado

, Steinman

R.M.

Virus replication begins in dendritic cells during the transmission of HIV-1 from mature dendritic cells to T cells. Curr Biol. 1999; 9: 21–9.

58.

Kawamura

Candidate microbicides block HIV-1 infection of human immature Langerhans cells within epithelial tissue explants. J Exp Med. 2000; 192: 1491–500.

59.

Patterson

, Rae

, Hockey

, Gilmour

, Gotch

Plasmacytoid dendritic cells are highly susceptible to human immunodeficiency virus type 1 infection and release infectious virus. J Virol. 2001; 75(14): 6710–3.

60.

Donaghy

Loss of blood CD11c+ myeloid and CD11c– plasmacytoid dendritic cells in patients with HIV-1 infection correlates with HIV-1 RNA virus load. Blood. 2001; 98: 2574–6.

61.

Smed-Sörensen

Differential susceptibility to human immunodeficiency virus type 1 infection of myeloid and plasmacytoid dendritic cells. J Virol. 2005; 79: 8861–9.

62.

Steinman

R.M.

, Granelli-Piperno

, Pope

The interaction of immunodeficiency viruses with dendritic cells. Curr Top Microbiol Immunol. 2003; 276: 1–30.

63.

Cameron

P.U.

, Forsum

, Teppler

, Granelli-Piperno

, Steinman

R.M.

During HIV-1 infection most blood dendritic cells are not productively infected and can induce allogeneic CD4+ T cells clonal expansion. Clin Exp Immunol. 1992; 88: 226–36.

64.

Pope

M.G.S.

, Gallo

, Hoffman

, Steinman

R.M.

Low levels of HIV-1 infection in cutaneous dendritic cells promote extensive viral replication upon binding to memory CD4+ T cells. J Exp Med. 1995; 182(6): 2045–56.

65.

McIlroy

Infection frequency of dendritic cells and CD4+ T lymphocytes in spleens of human immunodeficiency virus-positive patients. J Virol. 1995; 69: 4737–45.

66.

Canque

The susceptibility to X4 and R5 human immunodeficiency virus-1 strains of dendritic cells derived in vitro from CD34+ hematopoietic progenitor cells is primarily determined by their maturation stage. Blood. 1999; 93: 3866–75.

67.

Fong

, Mengozzi

, Abbey

N.W.

, Herndier

B.G.

, Engleman

E.G.

Productive infection of plasmacytoid dendritic cells with human immunodeficiency virus type 1 is triggered by CD40 ligation. J Virol. 2002; 76: 11033–41.

68.

Laskus

, Radkowski

, Wang

L.F.

, Nowicki

, Rakela

Uneven distribution of hepatitis C virus quasispecies in tissues from subjects with end-stage liver disease: confounding effect of viral adsorption and mounting evidence for the presence of low-level extrahepatic replication. J Virol. 2000; 74(2): 1014–7.

69.

Roque-Afonso

A-M

, Ducoulombier

, Di Liberto

Compartmentalization of hepatitis C virus genotypes between plasma and peripheral blood mononuclear cells. J Virol. 2005; 79(10): 6349–57.

70.

Pham

T.N.Q.

, MacParland

S.A.

, Mulrooney

P.M.

, Cooksley

, Naoumov

N.V.

, Michalak

T.I.

Hepatitis C virus persistence after spontaneous or treatment-induced resolution of hepatitis C. J Virol. 2004; 78(11): 5867–74.

71.

Radkowski

, Gallegos-Orozco

J.F.

, Jablonska

Persistence of hepatitis C virus in patients successfully treated for chronic hepatitis C. Hepatology. 2005; 41(1): 106–14.

72.

Carreño

, Pardo

, López-Alcorocho

J.M.

, Rodríguez-Iñigo

, Bartolomé

, Castillo

Detection of hepatitis c virus (HCV) RNA in the liver of healthy, anti-HCV Antibody-positive, serum HCV RNA-negative patients with normal alanine aminotransferase levels. J Infect Dis. 2006; 194(1): 53–60.

73.

De Felipe

, Leal

, Soriano-Sarabia

HCV RNA in peripheral blood cell subsets in HCV-HIV coinfected patients at the end of PegIFN/RBV treatment is associated with virologic relapse. Journal of Viral Hepatitis. 2009; 16(1): 21–7.

74.

Lee

W.M.

, Polson

J.E.

, Carney

D.S.

, Sahin

, Gale

Jr. . Reemergence of hepatitis C virus after 8.5 years in a patient with hypogammaglobulinemia: evidence for an occult viral reservoir. J Infect Dis. 2005; 192(6): 1088–92.

75.

Lin

, Thadareddy

, Goldstein

M.J.

, Lake-Bakaar

Immune suppression leading to hepatitis C virus re-emergence after sustained virological response. J Med Virol. 2008; 80(10): 1720–2.

76.

Goutagny

, Fatmi

, Ledinghen

V.D.

Evidence of viral replication in circulating dendritic cells during hepatitis C virus infection. The J Infect Dis. 2003; 187(12): 1951–8.

77.

Rodrigue-Gervais

I.G.

Poly(I: C) and lipopolysaccharide innate sensing functions of circulating human myeloid dendritic cells are affected in vivo in hepatitis C virus-infected patients. J Virol. 2007; 81: 5537–46.

78.

Navas

M.C.

Dendritic cell susceptibility to hepatitis C virus genotype 1 infection. J Med Virol. 2002; 67: 152–61.

79.

Liang

Differential effects of hepatitis C virus JFH1 on human myeloid and plasmacytoid dendritic cells. J Virol. 2009; 83: 5693–707.

80.

Shiina

, Rehermann

Cell culture-produced hepatitis C virus impairs plasmacytoid dendritic cell function. Hepatology. 2008; 47: 385–95.

81.

Marukian

Cell culture-produced hepatitis C virus does not infect peripheral blood mononuclear cells. Hepatology. 2008; 48: 1843–50.

82.

Cambi

, Koopman

, Figdor

C.G.

How C-type lectins detect pathogens. Cell Microbiol. 2005; 7: 481–8.

83.

Smith

A.L.

Leukocyte-specific protein 1 interacts with DC-SIGN and mediates transport of HIV to the proteasome in dendritic cells. J Exp Med. 2007; 204: 421–30.

84.

Moris

DC-SIGN promotes exogenous MHC-I-restricted HIV-1 antigen presentation. Blood. 2004; 103: 2648–54.

85.

Barth

Scavenger receptor class B is required for hepatitis C virus uptake and cross-presentation by human dendritic cells. J Virol. 2008; 82: 3466–79.

86.

Chiu

Y.L.

Cellular APOBEC3G restricts HIV-1 infection in resting CD4+ T cells. Nature. 2005; 435: 108–14.

87.

Kreisberg

J.F.

, Yonemoto

, Greene

W.C.

Endogenous factors enhance HIV infection of tissue naive CD4 T cells by stimulating high molecular mass APOBEC3G complex formation. J Exp Med. 2006; 203: 865–70.

88.

Kinoshita

, Chen

B.K.

, Kaneshima

, Nolan

G.P.

Host control of HIV-1 parasitism in T cells by the nuclear factor of activated T cells. Cell. 1998; 95: 595–604.

89.

Ganesh

The gene product Murr1 restricts HIV-1 replication in resting CD4+ lymphocytes. Nature. 2003; 426: 853–7.

90.

Lassen

K.G.

, Ramyar

K.X.

, Bailey

J.R.

, Zhou

, Siliciano

R.F.

Nuclear retention of multiply spliced HIV-1 RNA in resting CD4+ T cells. PLoS Pathog. 2006; 2: e68.

91.

Peng

Myeloid differentiation and susceptibility to HIV-1 are linked to APOBEC3 expression. Blood. 2007; 110: 393–400.

92.

Wang

F-X

, Huang

, Zhang

, Ma

, Zhang

APOBEC3G upregulation by alpha interferon restricts human immunodeficiency virus type 1 infection in human peripheral plasmacytoid dendritic cells. J Gen Virol. 2008; 89(3): 722–30.

93.

Lee

, Sharron

, Montaner

L.J.

, Weissman

, Doms

R.W.

Quantification of CD4, CCR5, and CXCR4 levels on lymphocyte subsets, dendritic cells, and differentially conditioned monocyte-derived macrophages. Proc Natl Acad Sci U S A. 1999; 96: 5215–20.

94.

Pohlmann

Hepatitis C virus glycoproteins interact with DC-SIGN and DC-SIGNR. J Virol. 2003; 77: 4070–80.

95.

Piguet

, Steinman

R.M.

The interaction of HIV with dendritic cells: outcomes and pathways. Trends Immunol. 2007; 28(11): 503–10.

96.

, KewalRamani

V.N.

Dendritic-cell interactions with HIV: infection and viral dissemination. Nat Rev Immunol. 2006; 6(11): 859–68.

97.

Blanchet

F.P.

, Moris

, Nikolic

D.S.

Human immunodeficiency virus-1 inhibition of immunoamphisomes in dendritic cells impairs early innate and adaptive immune responses. Immunity. 2010; 32(5): 654–69.

98.

Granelli-Piperno

, Shimeliovich

, Pack

, Trumpfheller

, Steinman

R.M.

HIV-1 selectively infects a subset of nonmaturing BDCA1-positive dendritic cells in human blood. J Immunol. 2006; 176(2): 991–8.

99.

Granelli-Piperno

, Golebiowska

, Trumpfheller

, Siegal

F.P.

, Steinman

R.M.

HIV-1-infected monocyte-derived dendritic cells do not undergo maturation but can elicit IL-10 production and T cell regulation. Proc Natl Acad Sci U S A. 2004; 101: 7669–74.

100.

Harman

A.N.

HIV-1-infected dendritic cells show 2 phases of gene expression changes, with lysosomal enzyme activity decreased during the second phase. Blood. 2009; 114: 85–94.

101.

Rubbert

, Combadiere

, Ostrowski

Dendritic cells express multiple chemokine receptors used as coreceptors for HIV entry. J Immunol. 1998; 160(8): 3933–41.

102.

Granelli-Piperno

Efficient interaction of HIV-1 with purified dendritic cells via multiple chemokine coreceptors. J Exp Med. 1996; 184: 2433–8.

103.

Ignatius

The immunodeficiency virus coreceptor, Bonzo/STRL33/ TYMSTR, is expressed by macaque and human skin- and blood-derived dendritic cells. AIDS Res Hum Retroviruses. 2000; 16: 1055–9.

104.

Geijtenbeek

T.B.

DC-SIGN, a dendritic cell-specific HIV-1-binding protein that enhances trans-infection of T cells. Cell. 2000; 100: 587–97.

105.

Piguet

, Sattentau

Dangerous liaisons at the virological synapse. J Clin Invest. 2004; 114: 605–10.

106.

Cavrois

, Neidleman

, Kreisberg

J.F.

, Greene

W.C.

In vitro derived dendritic cells trans-infect CD4 T cells primarily with surface-bound HIV-1 virions. PLoS Pathog. 2007; 3(1): e4.

107.

H.J.

, Reuter

M.A.

, McDonald

HIV Traffics through a specialized, surface-accessible intracellular compartment during trans-infection of T cells by mature dendritic cells. PLoS Pathog. 2008; 4(8): e1000134.

108.

Baribaud

, Pohlmann

, Leslie

, Mortari

, Doms

R.W.

Quantitative expression and virus transmission analysis of DC-SIGN on monocyte-derived dendritic cells. J Virol. 2002; 76: 9135–42.

109.

Granelli-Piperno

Dendritic cell-specific intercellular adhesion molecule 3-grabbing nonintegrin/CD209 is abundant on macrophages in the normal human lymph node and is not required for dendritic cell stimulation of the mixed leukocyte reaction. J Immunol. 2005; 175: 4265–73.

110.

Gummuluru

, Rogel

, Stamatatos

, Emerman

Binding of human immunodeficiency virus type 1 to immature dendritic cells can occur independently of DC-SIGN and mannose binding C-type lectin receptors via a cholesterol-dependent pathway. J Virol. 2003; 77: 12865–74.

111.

Trumpfheller

, Park

C.G.

, Finke

, Steinman

R.M.

, Granelli-Piperno

Cell type-dependent retention and transmission of HIV-1 by DC-SIGN. Int Immunol. 2003; 15: 289–98.

112.

, Bashirova

A.A.

, Martin

T.D.

Rhesus macaque dendritic cells efficiently transmit primate lentiviruses independently of DC-SIGN. Proc Natl Acad Sci U S A. 2002; 99(3): 1568–73.

113.

, Martin

T.D.

, Vazeux

, Unutmaz

, KewalRamani

V.N.

Functional evaluation of DC-SIGN monoclonal antibodies reveals DC-SIGN interactions with ICAM-3 do not promote human immunodeficiency virus type 1 transmission. J Virol. 2002; 76: 5905–14.

114.

Wang

J.H.

, Janas

A.M.

, Olson

W.J.

, Wu

Functionally distinct transmission of human immunodeficiency virus type 1 mediated by immature and mature dendritic cells. J Virol. 2007; 81(17): 8933–43.

115.

Sabatte

Human seminal plasma abrogates the capture and transmission of human immunodeficiency virus type 1 to CD4+ T cells mediated by DC-SIGN. J Virol. 2007; 81: 13723–34.

116.

Fahrbach

K.M.

, Barry

S.M.

, Ayehunie

, Lamore

, Klausner

, Hope

T.J.

Activated CD34-derived Langerhans cells mediate transinfection with human immunodeficiency virus. J Virol. 2007; 81(13): 6858–68.

117.

Ganesh

Infection of specific dendritic cells by CCR5-tropic human immunodeficiency virus type 1 promotes cell-mediated transmission of virus resistant to broadly neutralizing antibodies. J Virol. 2004; 78: 11980–7.

118.

Izquierdo-Useros

, Blanco

, Erkizia

Maturation of blood-derived dendritic cells enhances human immunodeficiency virus type 1 capture and transmission. J Virol. 2007; 81(14): 7559–70.

119.

McDonald

, Wu

, Bohks

S.M.

, KewalRamani

V.N.

, Unutmaz

, Hope

T.J.

Recruitment of HIV and its receptors to dendritic cell-T cell junctions. Science. 2003; 300(5623): 1295–7.

120.

Sanders

R.W.

Differential transmission of human immunodeficiency virus type 1 by distinct subsets of effector dendritic cells. J Virol. 2002; 76: 7812–21.

121.

Turville

S.G.

, Santos

J.J.

, Frank

Immunodeficiency virus uptake, turnover, and 2-phase transfer in human dendritic cells. Blood. 2004; 103(6): 2170–9.

122.

Wang

J-H

, Kwas

, Wu

Intercellular adhesion molecule 1 (ICAM-1), but not ICAM-2 and −3, is important for dendritic cell-mediated human immunodeficiency virus type 1 transmission. J Virol. 2009; 83(9): 4195–204.

123.

Dustin

M.L.

, Springer

T.A.

Role of lymphocyte adhesion receptors in transient interactions and cell locomotion. Annu Rev Immunol. 1991; 9: 27–66.

124.

Burleigh

Infection of dendritic cells (DCs), not DC-SIGN-mediated internalization of human immunodeficiency virus, is required for long-term transfer of virus to T cells. J Virol. 2006; 80: 2949–57.

125.

Wang

J.H.

, Janas

A.M.

, Olson

W.J.

, Kewal Ramani

V.N.

, Wu

CD4 coexpression regulates DC-SIGN-mediated transmission of human immunodeficiency virus type 1. J Virol. 2007; 81(5): 2497–507.

126.

Groot

, van Capel

T.M.

, Kapsenberg

M.L.

, Berkhout

, de Jong

E.C.

Opposing roles of blood myeloid and plasmacytoid dendritic cells in HIV-1 infection of T cells: transmission facilitation versus replication inhibition. Blood. 2006; 108: 1957–64.

127.

de Witte

Langerin is a natural barrier to HIV-1 transmission by Langerhans cells. Nature Med. 2007; 13: 367–71.

128.

Gardner

J.P.

L-SIGN (CD 209L) is a liver-specific capture receptor for hepatitis C virus. Proc Natl Acad Sci U S A. 2003; 100: 4498–503.

129.

Lozach

P.Y.

DC-SIGN and L-SIGN are high affinity binding receptors for hepatitis C virus glycoprotein E2. J Biol Chem. 2003; 278: 20358–66.

130.

Cormier

E.G.

L-SIGN (CD209L) and DC-SIGN (CD209) mediate transinfection of liver cells by hepatitis C virus. Proc Natl Acad Sci U S A. 2004; 101: 14067–72.

131.

Ludwig

I.S.

Hepatitis C virus targets DC-SIGN and L-SIGN to escape lysosomal degradation. J Virol. 2004; 78: 8322–32.

132.

Lai

W.K.

Expression of DC-SIGN and DC-SIGNR on human sinusoidal endothelium: a role for capturing hepatitis C virus particles. Am J Pathol. 2006; 169: 200–8.

133.

Pacanowski

Reduced blood CD123+ (lymphoid) and CD11c+(myeloid) dendritic cell numbers in primary HIV-1 infection. Blood. 2001; 98: 3016–21.

134.

Grassi

Depletion in blood CD11c-positive dendritic cells from HIV-infected patients. AIDS. 1999; 13: 759–66.

135.

Chehimi

Persistent decreases in blood plasmacytoid dendritic cell number and function despite effective highly active antiretroviral therapy and increased blood myeloid dendritic cells in HIV-infected individuals. J Immunol. 2002; 168: 4796–801.

136.

Soumelis

, Scott

, Gheyas

Depletion of circulating natural type 1 interferon-producing cells in HIV-infected AIDS patients. Blood. 2001; 98(4): 906–12.

137.

Cavaleiro

Major depletion of plasmacytoid dendritic cells in HIV-2 infection, an attenuated form of HIV disease. PLoS Pathog. 2009; 5: e1000667.

138.

Ulsenheimer

Plasmacytoid dendritic cells in acute and chronic hepatitis C virus infection. Hepatology. 2005; 41: 643–51.

139.

Wertheimer

A.M.

, Bakke

, Rosen

H.R.

Direct enumeration and functional assessment of circulating dendritic cells in patients with liver disease. Hepatology. 2004; 40: 335–45.

140.

Longman

R.S.

, Talal

A.H.

, Jacobson

I.M.

, Rice

C.M.

, Albert

M.L.

Normal functional capacity in circulating myeloid and plasmacytoid dendritic cells in patients with chronic hepatitis C. J Infect Dis. 2005; 192: 497–503.

141.

Kanto

Reduced numbers and impaired ability of myeloid and plasmacytoid dendritic cells to polarize T helper cells in chronic hepatitis C virus infection. J Infect Dis. 2004; 190: 1919–26.

142.

Nattermann

, Zimmermann

, Iwan

Hepatitis C virus E2 and CD81 interaction may be associated with altered trafficking of dendritic cells in chronic hepatitis C. Hepatology. 2006; 44(4): 945–54.

143.

Dolganiuc

Hepatitis C virus (HCV) core protein-induced, monocytemediated mechanisms of reduced IFN-α and plasmacytoid dendritic cell loss in chronic HCV infection. J Immunol. 2006; 177: 6758–68.

144.

Meyers

J.H.

Impact of HIV on cell survival and antiviral activity of plasmacytoid dendritic cells. PLoS One. 2007; 2: e458.

145.

Brown

K.N.

, Wijewardana

, Liu

, Barratt-Boyes

S.M.

Rapid influx and death of plasmacytoid dendritic cells in lymph nodes mediate depletion in acute simian immunodeficiency virus infection. PLoS Pathog. 2009; 5: e1000413.

146.

Zhang

Severe dendritic cell perturbation is actively involved in the pathogenesis of acute-on-chronic hepatitis B liver failure. J Hepatol. 2008; 49: 396–406.

147.

Lai

W.K.

Hepatitis C is associated with perturbation of intrahepatic myeloid and plasmacytoid dendritic cell function. J Hepatol. 2007; 47: 338–47.

148.

Sansonno

, Lotesoriere

, Cornacchiulo

Hepatitis C virus infection involves CD34+ hematopoietic progenitor cells in hepatitis C virus chronic carriers. Blood. 1998; 92(9): 3328–37.

149.

Siavoshian

, Abraham

J.D.

, Thumann

, Kieny

M.P.

, Schuster

Hepatitis C virus core, NS3, NS5A, NS5B proteins induce apoptosis in mature dendritic cells. J Med Virol. 2005; 75(3): 402–11.

150.

Chehimi

Impaired interleukin 12 production in human immunodeficiency virus-infected patients. J Exp Med. 1994; 179: 1361–6.

151.

Chougnet

C.A.

, Margolis

, Landay

A.L.

, Kessler

H.A.

, Shearer

G.M.

Contribution of prostaglandin E2 to the interleukin-12 defect in HIV-infected patients. AIDS. 1996; 10: 1043–5.

152.

Donaghy

, Gazzard

, Gotch

, Patterson

Dysfunction and infection of freshly isolated blood myeloid and plasmacytoid dendritic cells in patients infected with HIV-1. Blood. 2003; 101: 4505–11.

153.

Kanto

Impaired allostimulatory capacity of peripheral blood dendritic cells recovered from hepatitis C virus-infected individuals. J Immunol. 1999; 162: 5584–91.

154.

Dolganiuc

Hepatitis C virus core and nonstructural protein 3 proteins induce pro- and anti-inflammatory cytokines and inhibit dendritic cell differentiation. J Immunol. 2003; 170: 5615–24.

155.

Chehimi

Baseline viral load and immune activation determine the extent of reconstitution of innate immune effectors in HIV-1-infected subjects undergoing antiretroviral treatment. J Immunol. 2007; 179: 2642–50.

156.

Conry

S.J.

Impaired plasmacytoid dendritic cell (PDC)-NK cell activity in viraemic human immunodeficiency virus infection attributable to impairments in both PDC and NK cell function. J Virol. 2009; 83: 11175–87.

157.

Auffermann-Gretzinger

, Keeffe

E.B.

, Levy

Impaired dendritic cell maturation in patients with chronic, but not resolved, hepatitis C virus infection. Blood. 2001; 97: 3171–6.

158.

Bain

, Fatmi

, Zoulim

, Zarski

J.P.

, Trepo

, Inchauspe

Impaired allostimulatory function of dendritic cells in chronic hepatitis C infection. Gastroenterology. 2001; 120(2): 512–24.

159.

Dolganiuc

, Paek

, Kodys

, Thomas

, Szabo

Myeloid dendritic cells of patients with chronic HCV infection induce proliferation of regulatory T lymphocytes. Gastroenterology. 2008; 135: 2119–27.

160.

Kamga

Type I interferon production is profoundly and transiently impaired in primary HIV-1 infection. J Infect Dis. 2005; 192: 303–10.

161.

Mengshol

J.A.

, Golden-Mason

, Castelblanco

Impaired plasmacytoid dendritic cell maturation and differential chemotaxis in chronic hepatitis C virus: associations with antiviral treatment outcomes. Gut. 2009; 58(7): 964–73.

162.

Martinelli

HIV-1 gp120 inhibits TLR9-mediated activation and IFN-α secretion in plasmacytoid dendritic cells. Proc Natl Acad Sci U S A. 2007; 104: 3396–401.

163.

HBsAg inhibits TLR9-mediated activation and IFN-α production in plasmacytoid dendritic cells. Mol Immunol. 2009; 46: 2640–6.

164.

Gondois-Rey

Hepatitis C virus is a weak inducer of interferon alpha in plasmacytoid dendritic cells in comparison with influenza and human herpesvirus type-1. PLoS One. 2009; 4: e4319.

165.

Takahashi

, Asabe

, Wieland

Plasmacytoid dendritic cells sense hepatitis C virus, infected cells, produce interferon, and inhibit infection. Proc Natl Acad Sci U S A. 2010; 107(16): 7431–6.

166.

A.I.

, Pezacki

J.P.

, Wodicka

Genomic analysis of the host response to hepatitis C virus infection. Proc Natl Acad Sci U S A. 2002; 99(24): 15669–74.

167.

Bigger

C.B.

, Guerra

, Brasky

K.M.

Intrahepatic Gene Expression during Chronic Hepatitis C Virus Infection in Chimpanzees. J Virol. 2004; 78(24): 13779–92.

168.

Rehermann

Hepatitis C virus versus innate and adaptive immune responses: a tale of coevolution and coexistence. J Clin Invest. 2009; 119(7): 1745–54.

169.

Chen

, Liang

, Peterson

A.J.

, Munn

D.H.

, Blazar

B.R.

The indoleamine 2,3-dioxygenase pathway is essential for human plasmacytoid dendritic cell-induced adaptive T regulatory cell generation. J Immunol. 2008; 181(8): 5396–404.

170.

Boasso

, Herbeuval

J-P

, Hardy

A.W.

HIV inhibits CD4+ T-cell proliferation by inducing indoleamine 2,3-dioxygenase in plasmacytoid dendritic cells. Blood. 2007; 109(8): 3351–9.

171.

Manches

, Munn

, Fallahi

HIV-activated human plasmacytoid DCs induce Tregs through an indoleamine 2,3-dioxygenase-dependent mechanism. J Clin Invest. 2008; 118(10): 3431–9.

172.

Vejbaesya

, Songsivilai

, Tanwandee

, Rachaibun

, Chantangpol

, Dharakul

HLA association with hepatitis C virus infection. Hum Immunol. 2000; 61(3): 348–53.

173.

Fernandez

N.C.

Dendritic cells directly trigger NK cell functions: crosstalk relevant in innate anti-tumor immune responses in vivo. Nature Med. 1999; 5: 405–11.

174.

Kikuchi

Dendritic cells pulsed with live and dead Legionella pneumophila elicit distinct immune responses. J Immunol. 2004; 172: 1727–34.

175.

Gerosa

Reciprocal activating interaction between natural killer cells and dendritic cells. J Exp Med. 2002; 195: 327–33.

176.

Gerosa

The reciprocal interaction of NK cells with plasmacytoid or myeloid dendritic cells profoundly affects innate resistance functions. J Immunol. 2005; 174: 727–34.

177.

Borg

NK cell activation by dendritic cells (DCs) requires the formation of a synapse leading to IL-12 polarization in DCs. Blood. 2004; 104: 3267–75.

178.

Martin-Fontecha

Induced recruitment of NK cells to lymph nodes provides IFN-γ for TH1 priming. Nature Immunol. 2004; 5: 1260–5.

179.

Piccioli

, Sbrana

, Melandri

, Valiante

N.M.

Contact-dependent stimulation and inhibition of dendritic cells by natural killer cells. J Exp Med. 2002; 195: 335–41.

180.

Ferlazzo

Distinct roles of IL-12 and IL-15 in human natural killer cell activation by dendritic cells from secondary lymphoid organs. Proc Natl Acad Sci U S A. 2004; 101: 16606–11.

181.

Ferlazzo

Human dendritic cells activate resting natural killer (NK) cells and are recognized via the NKp30 receptor by activated NK cells. J Exp Med. 2002; 195: 343–51.

182.

Reitano

K.N.

Defective plasmacytoid dendritic cell-NK cell cross-talk in HIV infection. AIDS Res Hum Retroviruses. 2009; 25: 1029–37.

183.

Tasca

Escape of monocyte-derived dendritic cells of HIV-1 infected individuals from natural killer cell-mediated lysis. AIDS. 2003; 17: 2291–8.

184.

Mavilio

Characterization of the defective interaction between a subset of natural killer cells and dendritic cells in HIV-1 infection. J Exp Med. 2006; 203: 2339–50.

185.

Quaranta

M.G.

HIV-1 Nef impairs the dynamic of DC/NK crosstalk: different outcome of CD56dim and CD56bright NK cell subsets. FASEB J. 2007; 21: 2323–34.

186.

Poggi

NK cell activation by dendritic cells is dependent on LFA-1-mediated induction of calcium-calmodulin kinase II: inhibition by HIV-1 Tat C-terminal domain. J Immunol. 2002; 168: 95–101.

187.

Melki

M.T.

, Saidi

, Dufour

, Olivo-Marin

J.C.

, Gougeon

M.L.

Escape of HIV-1-infected dendritic cells from TRAIL-mediated NK cell cytotoxicity during NK-DC cross-talk—a pivotal role of HMGB1. PLoS Pathog. 2010; 6: e1000862.

188.

Saidi

, Melki

M.T.

, Gougeon

M.L.

HMGB1-dependent triggering of HIV-1 replication and persistence in dendritic cells as a consequence of NK-DC cross-talk. PLoS One. 2008; 3: e3601.

189.

Alter

IL-10 induces aberrant deletion of dendritic cells by natural killer cells in the context of HIV infection. J Clin Invest. 2010; 120: 1905–13.

190.

Morishima

, Paschal

D.M.

, Wang

C.C.

Decreased NK cell frequency in chronic hepatitis C does not affect ex vivo cytolytic killing. Hepatology. 2006; 43(3): 573–80.

191.

Bonorino

, Ramzan

, Camous

Fine characterization of intrahepatic NK cells expressing natural killer receptors in chronic hepatitis B and C. J Hepatol. 2009; 51(3): 458–67.

192.

Dessouki

, Kamiya

, Nagahama

Chronic hepatitis C viral infection reduces NK cell frequency and suppresses cytokine secretion: Reversion by anti-viral treatment. Biochem Biophys Res Commun. 2010; 393(2): 331–7.

193.

Meier

U.C.

, Owen

R.E.

, Taylor

Shared alterations in NK cell frequency, phenotype, and function in chronic human immunodeficiency virus and hepatitis C virus infections. J Virol. 2005; 79(19): 12365–74.

194.

Oliviero

, Varchetta

, Paudice

Natural killer cell functional dichotomy in chronic hepatitis B and chronic hepatitis C virus infections. Gastroenterology. 2009; 137(3): 1151–1160, 1160 e1151–7.

195.

Appasamy

, Bryant

, Hassanein

, Van Thiel

D.H.

, Whiteside

T.L.

Effects of therapy with interferon-α on peripheral blood lymphocyte subsets and NK activity in patients with chronic hepatitis C. Clin Immunol Immunopathol. 1994; 73(3): 350–7.

196.

Bonavita

MS F.A.

, Paroli

Normalization of depressed natural killer activity after interferon-alpha therapy is associated with a low frequency of relapse in patients with chronic hepatitis C. Int J Tissue React. 1993; 15: 11–6.

197.

Golden-Mason

, Madrigal-Estebas

, McGrath

Altered natural killer cell subset distributions in resolved and persistent hepatitis C virus infection following single source exposure. Gut. 2008; 57(8): 1121–8.

198.

Jinushi

, Takehara

, Tatsumi

Autocrine/paracrine IL-15 that is required for type I IFN-mediated dendritic cell expression of MHC class I-related chain A and B is impaired in hepatitis C virus infection. J Immunol. 2003; 171(10): 5423–9.

199.

Nattermann

, Nischalke

H.D.

, Hofmeister

The HLA-A2 restricted T cell epitope HCV core 35–44 stabilizes HLA-E expression and inhibits cytolysis mediated by natural killer cells. Am J Pathol. 2005; 166(2): 443–53.

200.

Kupfer

, Kupfer

Imaging immune cell interactions and functions: SMACs and the Immunological Synapse. Seminars in Immunology. 2003; 15(6): 295–300.

201.

Rodriguez-Fernandez

J.L.

, Corbi

A.L.

Adhesion molecules in human dendritic cells. Curr Opin Investig Drugs. 2005; 6(11): 1103–11.

202.

Stoll

, Delon

, Brotz

T.M.

, Germain

R.N.

Dynamic imaging of T cell-dendritic cell interactions in lymph nodes. Science. 2002; 296(5574): 1873–6.

203.

Delon

, Stoll

, Germain

R.N.

Imaging of T-cell interactions with antigen presenting cells in culture and in intact lymphoid tissue. Immunol Rev. 2002; 189: 51–63.

204.

Huppa

J.B.

, Gleimer

, Sumen

, Davis

M.M.

Continuous T cell receptor signaling required for synapse maintenance and full effector potential. Nat Immunol. 2003; 4(8): 749–55.

205.

Mempel

T.R.

, Henrickson

S.E.

, Von Andrian

U.H.

T-cell priming by dendritic cells in lymph nodes occurs in three distinct phases. Nature. 2004; 427(6970): 154–9.

206.

Benvenuti

, Lagaudriere-Gesbert

, Grandjean

Dendritic cell maturation controls adhesion, synapse formation, and the duration of the interactions with naive T lymphocytes. J Immunol. 2004; 172(1): 292–301.

207.

Blaak

In vivo HIV-1 infection of CD45RA+CD4+ T cells is established primarily by syncytium-inducing variants and correlates with the rate of CD4+ T cell decline. Proc Natl Acad Sci U S A. 2000; 97: 1269–74.

208.

Ostrowski

M.A.

Both memory and CD45RA+/CD62L+ naive CD4+ T cells are infected in human immunodeficiency virus type 1-infected individuals. J Virol. 1999; 73: 6430–5.

209.

Zhang

Sexual transmission and propagation of SIV and HIV in resting and activated CD4+ T cells. Science. 1999; 286: 1353–7.

210.

Haase

A.T.

Perils at mucosal front lines for HIV and SIV and their hosts. Nature Rev Immunol. 2005; 5: 783–92.

211.

Williams

S.A.

NF-[kappa]B p50 promotes HIV latency through HDAC recruitment and repression of transcriptional initiation. EMBO J. 2006; 25: 139–49.

212.

Jordan

, Bisgrove

, Verdin

HIV reproducibly establishes a latent infection after acute infection of T cells in vitro. EMBO J. 2003; 22: 1868–77.

213.

Tong-Starksen

S.E.

, Luciw

P.A.

, Peterlin

B.M.

Human immunodeficiency virus long terminal repeat responds to T-cell activation signals. Proc Natl Acad Sci U S A. 1987; 84: 6845–9.

214.

Adams

Cellular latency in human immunodeficiency virus-infected individuals with high CD4 levels can be detected by the presence of promoter-proximal transcripts. Proc Natl Acad Sci U S A. 1994; 91: 3862–6.

215.

Arnold

, Brenner

, Becker

, Frey

C.R.

, Krammer

P.H.

How T lymphocytes switch between life and death. Eur J Immunol. 2006; 36: 1654–8.

216.

Bourgeois

, Stockinger

T cell homeostasis in steady state and lymphopenic conditions. Immunol Lett. 2006; 107: 89–92.

217.

Fackler

O.T.

, Alcover

, Schwartz

Modulation of the immunological synapse: a key to HIV-1 pathogenesis?

Nat Rev Immunol. 2007; 7(4): 310–17.

218.

Simmons

, Aluvihare

, McMichael

Nef triggers a transcriptional program in T cells imitating single-signal T cell activation and inducing HIV virulence mediators. Immunity. 2001; 14: 763–77.

219.

Wang

J.K.

, Kiyokawa

, Verdin

, Trono

The Nef protein of HIV-1 associates with rafts and primes T cells for activation. Proc Natl Acad Sci U S A. 2000; 97: 394–9.

220.

Fenard

Nef is physically recruited into the immunological synapse and potentiates T cell activation early after TCR engagement. J Immunol. 2005; 175: 6050–7.

221.

Fortin

J.F.

, Barat

, Beausejour

, Barbeau

, Tremblay

M.J.

Hyper-responsiveness to stimulation of human immunodeficiency virus-infected CD4+ T cells requires Nef and Tat virus gene products and results from higher NFAT, NF-kappaB, and AP-1 induction. J Biol Chem. 2004; 279(38): 39520–31.

222.

Keppler

O.T.

, Tibroni

, Venzke

, Rauch

, Fackler

O.T.

Modulation of specific surface receptors and activation sensitization in primary resting CD4+ T lymphocytes by the Nef protein of HIV-1. J Leukoc Biol. 2006; 79: 616–27.

223.

Thoulouze

M.I.

Human immunodeficiency virus type-1 infection impairs the formation of the immunological synapse. Immunity. 2006; 24: 547–61.

224.

Haller

The HIV-1 pathogenicity factor Nef interferes with maturation of stimulatory T-lymphocyte contacts by modulation of N-Wasp activity. J Biol Chem. 2006; 281: 19618–30.

225.

Rabi

S.A.

, O'Connell

K.A.

, Nikolaeva

Unstimulated primary CD4+ T cells from HIV-1-positive elite suppressors are fully susceptible to HIV-1 entry and productive infection. J Virol. 2011; 85(2): 979–86.

226.

Sáez-Cirión

, Pancino

, Sinet

, Venet

, Lambotte

HIV controllers: how do they tame the virus?

Trends Immunol. 2007; 28(12): 532–40.

227.

Dillon

S.M.

, Friedlander

L.J.

, Rogers

L.M.

Blood myeloid dendritic cells from HIV-1-infected individuals display a proapoptotic profile characterized by decreased Bcl-2 levels and by Caspase-3+ frequencies that are associated with levels of plasma viremia and T cell activation in an exploratory study. J Virol. 2011; 85(1): 397–409.

228.

Madhuri

, Manisha

, Meera

, Ramesh

Irreversible loss of pDCs by apoptosis during early HIV infection may be a critical determinant of immune dysfunction. Viral Immunol. 2010; 23(3): 241+.

229.

Laforge

, Campillo-Gimenez

, Monceaux

HIV/SIV infection primes monocytes and dendritic cells for apoptosis. PLoS Pathog. 2011; 7(6): e1002087.

230.

Riol-Blanco

, Delgado-Martin

, Sanchez-Sanchez

Immunological synapse formation inhibits, via NF-[kappa]B and FOXO1, the apoptosis of dendritic cells. Nat Immunol. 2009; 10(7): 753–60.

231.

Perez

O.D.

, Kinoshita

, Hitoshi

Activation of the PKB/AKT pathway by ICAM-2. Immunity. 2002; 16(1): 51–65.

232.

Tedder

J.C.P.

, Haas

K.M.

CD22: a multifunctional receptor that regulates B lymphocyte survival and signal transduction. Adv Immunol. 2005; 88: 1–50.

233.

Miga

A.J.

, Masters

S.R.

, Durell

B.G.

Dendritic cell longevity and T cell persistence is controlled by CD154-CD40 interactions. Eur J Immunol. 2001; 31(3): 959–65.

234.

Aicher

, Shu

G.L.

, Magaletti

Differential role for p38 mitogenactivated protein kinase in regulating CD40-induced gene expression in dendritic cells and B cells. J Immunol. 1999; 163(11): 5786–95.

235.

Chehimi

, Papasavvas

, Tomescu

Inability of plasmacytoid dendritic cells to directly lyse HIV-infected autologous CD4+ T cells despite induction of tumor necrosis factor-related apoptosis-inducing ligand. J Virol. 2010; 84(6): 2762–73.

236.

Herbeuval

J.P.

, Boasso

, Grivel

J.C.

TNF-related apoptosis-inducing ligand (TRAIL) in HIV-1-infected patients and its in vitro production by antigen-presenting cells. Blood. 2005; 105(6): 2458–64.

237.

Herbeuval

J.P.

Differential expression of IFN-α and TRAIL/DR5 in lymphoid tissue of progressor versus nonprogressor HIV-1-infected patients. Proc Natl Acad Sci U S A. 2006; 103: 7000–5.

238.

Herbeuval

J.P.

Regulation of TNF-related apoptosis-inducing ligand on primary CD4+ T cells by HIV-1: role of type I IFN-producing plasmacytoid dendritic cells. Proc Natl Acad Sci U S A. 2005; 102: 13974–9.

239.

Kim

, Dabrowska

, Jenner

R.G.

, Aldovini

Human and simian immunodeficiency virus-mediated upregulation of the apoptotic factor TRAIL occurs in antigen-presenting cells from AIDS-susceptible but not from AIDS-resistant species. J Virol. 2007; 81: 7584–97.

240.

Stary

, Klein

, Kohlhofer

Plasmacytoid dendritic cells express TRAIL and induce CD4+ T-cell apoptosis in HIV-1 viremic patients. Blood. 2009; 114(18): 3854–63.

241.

Bouma

, Mendoza-Naranjo

, Blundell

M.P.

Cytoskeletal remodeling mediated by WASp in dendritic cells is necessary for normal immune synapse formation and T-cell priming. Blood. 2011; 118(9): 2492–501.

242.

Borg

, Jalil

, Laderach

NK cell activation by dendritic cells (DCs) requires the formation of a synapse leading to IL-12 polarization in DCs. Blood. 2004; 104(10): 3267–75.

243.

Haller

, Rauch

, Michel

The HIV-1 Pathogenicity factor nef interferes with maturation of stimulatory T-lymphocyte contacts by modulation of N-Wasp activity. J Biol Chem. 2006; 281(28): 19618–30.

244.

Swingler

HIV-1 Nef mediates lymphocyte chemotaxis and activation by infected macrophages. Nature Med. 1999; 5: 997–1003.

245.

Messmer

, Jacque

J.M.

, Santisteban

Endogenously expressed nef uncouples cytokine and chemokine production from membrane phenotypic maturation in dendritic cells. J Immunol. 2002; 169(8): 4172–82.

246.

Briggs

S.D.

, Scholtz

, Jacque

J.M.

, Swingler

, Stevenson

, Smithgall

T.E.

HIV-1 Nef promotes survival of myeloid cells by a Stat3-dependent pathway. J Biol Chem. 2001; 276(27): 25605–11.

247.

Percario

Human immunodeficiency virus type 1 (HIV-1) Nef activates STAT3 in primary human monocyte/macrophages through the release of soluble factors: involvement of Nef domains interacting with the cell endocytotic machinery. J Leukoc Biol. 2003; 74: 821–32.

248.

Sarobe

, Lasarte

J.J.

, Casares

Abnormal priming of CD4(+) T cells by dendritic cells expressing hepatitis C virus core and E1 proteins. J Virol. 2002; 76(10): 5062–70.

249.

Zimmermann

, Flechsig

, La Monica

, Tripodi

, Adler

, Dikopoulos

Hepatitis C virus core protein impairs in vitro priming of specific T cell responses by dendritic cells and hepatocytes. J Hepatol. 2008; 48(1): 51–60.

250.

Krishnadas

D.K.

, Ahn

J.S.

, Han

, Kumar

, Agrawal

Immunomodulation by hepatitis C virus-derived proteins: targeting human dendritic cells by multiple mechanisms. Int Immunol. 2010; 22(6): 491–502.

251.

Crispe

I.N.

The liver as a lymphoid organ. Annu Rev Immunol. 2009; 27: 147–63.

252.

Qian

Murine liver allograft transplantation: tolerance and donor cell chimerism. Hepatology. 1994; 19: 916–24.

253.

Sumpter

T.L.

, Abe

, Tokita

, Thomson

A.W.

Dendritic cells, the liver, and transplantation. Hepatology. 2007; 46: 2021–31.

254.

Radziewicz

Liver-infiltrating lymphocytes in chronic human hepatitis C virus infection display an exhausted phenotype with high levels of PD-1 and low levels of CD127 expression. J Virol. 2007; 81: 2545–53.

255.

Warren

T lymphocytes interact with hepatocytes through fenestrations in murine liver sinusoidal endothelial cells. Hepatology. 2006; 44: 1182–90.

256.

Dienes

H.P.

, Hutteroth

, Hess

, Meuer

S.C.

Immunoelectron microscopic observations on the inflammatory infiltrates and HLA antigens in hepatitis B and non-A, non-B. Hepatology. 1987; 7: 1317–25.

257.

Franco

Expression of class I and class II major histocompatibility complex antigens on human hepatocytes. Hepatology. 1988; 8: 449–54.

258.

Bertolino

, Trescol-Biemont

M.C.

, Rabourdin-Combe

Hepatocytes induce functional activation of naive CD8+ T lymphocytes but fail to promote survival. Eur J Immunol. 1998; 28: 221–36.

259.

Bowen

D.G.

The site of primary T cell activation is a determinant of the balance between intrahepatic tolerance and immunity. J Clin Invest. 2004; 114: 701–12.

260.

Greten

T.F.

, Slansky

J.E.

, Kubota

Direct visualization of antigen-specific T cells: HTLV-1 Tax11-19- specific CD8(+) T cells are activated in peripheral blood and accumulate in cerebrospinal fluid from HAM/TSP patients. Proc Natl Acad Sci U S A. 1998; 95(13): 7568–73.

261.

Nischalke

H-D

, Coenen

, Berger

The toll-like receptor 2 (TLR2) −196 to −174 del/ins polymorphism affects viral loads and susceptibility to hepatocellular carcinoma in chronic hepatitis C. International Journal of Cancer. 2012; 130(6): 1470–5.

262.

Medhi

, Deka

Promoter region polymorphism and expression profile of toll like receptor-3 (TLR-3) gene in chronic hepatitis C virus (HCV) patients from India. Indian J Med Res. 2011; 134(2): 200–7.

263.

Askar

, Bregadze

, Mertens

TLR3 gene polymorphisms and liver disease manifestations in chronic hepatitis C. J Med Virol. 2009; 81(7): 1204–11.

264.

Schott

, Witt

, Neumann

Association of TLR7 single nucleotide polymorphisms with chronic HCV-infection and response to interferon-a-based therapy. J Viral Hepat. 2008; 15(1): 71–8.

265.

Schott

, Witt

, Neumann

A Toll-like receptor 7 single nucleotide polymorphism protects from advanced inflammation and fibrosis in male patients with chronic HCV-infection. J Hepatol. 2007; 47(2): 203–11.

266.

Askar

, Ramadori

, Mihm

Toll-like receptor 7 rs179008/Gln11 Leu gene variants in chronic hepatitis C virus infection. J Med Virol. 2010; 82(11): 1859–68.

267.

Wang

C.H.

, Eng

H.L.

, Lin

K.H.

TLR7 and TLR8 gene variations and susceptibility to hepatitis C virus infection. PLoS One. 2011; 6(10): e26235.

268.

Wietzke-Braun

, Maouzi

A.B.

, Manhardt

L.B.

, Bickeboller

, Ramadori

, Mihm

Interferon regulatory factor-1 promoter polymorphism and the outcome of hepatitis C virus infection. Eur J Gastroenterol Hepatol. 2006; 18(9): 991–7.

269.

Sermasathanasawadi

, Kato

, Muroyama

Association of interferon regulatory factor-7 gene polymorphism with liver cirrhosis in chronic hepatitis C patients. Liver International. 2008; 28(6): 798–806.

270.

Sironi

, Biasin

, Cagliani

A common polymorphism in TLR3 confers natural resistance to HIV-1 infection. J Immunol. 2012; 188(2): 818–23.

271.

Pine

S.O.

, McElrath

M.J.

, Bochud

P.Y.

Polymorphisms in toll-like receptor 4 and toll-like receptor 9 influence viral load in a seroincident cohort of HIV-1-infected individuals. AIDS. 2009; 23(18): 2387–95.

272.

DYBK

, Hamouda

, Eckert

J.K.

A frequent functional toll-like receptor 7 polymorphism is associated with accelerated HIV-1 disease progression. AIDS. 2009; 23(3): 297–307.

273.

Siddiqui

R.A.

, Krawczak

, Platzer

, Sauermann

Association of TLR7 variants with AIDS-like disease and AIDS vaccine efficacy in rhesus macaques. PLoS One. 2011; 6(10): e25474.

274.

D-Y

, Taube

, Hamouda

A functional toll-like receptor 8 variant is associated with HIV disease restriction. J Infect Dis. 2008; 198(5): 701–9.

275.

Bochud

P-YAB

, Hersberger

M.G.

, Taffe

P.E.F.

Polymorphisms in Toll-like receptor 9 influence the clinical course of HIV-1 infection. AIDS. 2007; 21(4): 441–6.

276.

Soriano-Sarabia

, Vallejo

, Ramirez-Lorca

Influence of the Toll-like receptor 9 1635A/G polymorphism on the CD4 count, HIV viral load, and clinical progression. J Acquir Immune Defic Syndr. 2008; 49(2): 128–35.

277.

Ricci

, Malacrida

, Zanchetta

Toll-like receptor 9 polymorphisms influence mother-to-child transmission of human immunodeficiency virus type 1. J Transl Med. 2010; 8: 49.

278.

Ball

T.B.

, Ji

, Kimani

Polymorphisms in IRF-1 associated with resistance to HIV-1 infection in highly exposed uninfected Kenyan sex workers. AIDS. 2007; 21(9): 1091–101.

279.

Chang

, Lindsay

R.J.

, Kulkarni

, Lifson

J.D.

, Carrington

, Altfeld

Polymorphisms in interferon regulatory factor 7 reduce interferon-alpha responses of plasmacytoid dendritic cells to HIV-1. AIDS. 2011; 25(5): 715–7.

280.

Yoon

S.K.

, Han

J.Y.

, Pyo

C-W

. Association between human leukocytes antigen alleles and chronic hepatitis C virus infection in the Korean population. Liver Int. 2005; 25(6): 1122–7.

281.

Alric

, Fort

, Izopet

Study of host- and virus-related factors associated with spontaneous hepatitis C virus clearance. Tissue Antigens. 2000; 56(2): 154–8.

282.

Wang

J.H.

, Zheng

, Ke

Ethnic and geographical differences in HLA associations with the outcome of hepatitis C virus infection. Virol J. 2009; 6: 46.

283.

McKiernan

S.M.

, Hagan

, Curry

The MHC is a major determinant of viral status, but not fibrotic stage, in individuals infected with hepatitis C. Gastroenterology. 2000; 118(6): 1124–30.

284.

Harris

R.A.

, Sugimoto

, Kaplan

D.E.

, Ikeda

, Kamoun

, Chang

K-M

. Human leukocyte antigen class II associations with hepatitis C virus clearance and virus-specific CD4 T cell response among Caucasians and African Americans. Hepatology. 2008; 48(1): 70–9.

285.

Thio

C.L.

, Gao

, Goedert

J.J.

HLA-Cw*04 and hepatitis C virus persistence. J Virol. 2002; 76(10): 4792–7.

286.

Wawrzynowicz-Syczewska

, Underhill

J.A.

, Clare

M.A.

, Boron-Kaczmarska

, McFarlane

I.G.

, Donaldson

P.T.

HLA class II genotypes associated with chronic hepatitis C virus infection and response to alpha-interferon treatment in Poland. Liver. 2000; 20(3): 234–9.

287.

Romero

, Azocar

, Zuniga

Interaction of NK inhibitory receptor genes with HLA-C and MHC class II alleles in hepatitis C virus infection outcome. Mol Immunol. 2008; 45(9): 2429–36.

288.

Fanning

L.J.

, Levis

, Kenny-Walsh

, Wynne

, Whelton

, Shanahan

Viral clearance in hepatitis C (1b) infection: Relationship with human leukocyte antigen class II in a homogeneous population. Hepatology. 2000; 31(6): 1334–7.

289.

Barrett

, Goh

, Coughlan

The natural course of hepatitis C virus infection after 22 years in a unique homogenous cohort: spontaneous viral clearance and chronic HCV infection. Gut. 2001; 49(3): 423–30.

290.

McKiernan

S.M.

, Hagan

, Curry

Distinct MHC class I and II alleles are associated with hepatitis C viral clearance, originating from a single source. Hepatology. 2004; 40(1): 108–14.

291.

Ksiaa

, Ayed-Jendoubi

, Sfar

Clearance and persistence of hepatitis C virus in a Tunisian population: association with HLA class I and class II. Viral Immunol. 2007; 20(2): 312–9.

292.

Yenigun

, Durupinar

Decreased frequency of the HLA-DRB1*11 allele in patients with chronic hepatitis C virus infection. J Virol. 2002; 76(4): 1787–9.

293.

Barrett

, Ryan

, Crowe

Association of the HLA-DRB1*01 allele with spontaneous viral clearance in an Irish cohort infected with hepatitis C virus via contaminated anti-D immunoglobulin. J Hepatol. 1999; 30(6): 979–83.

294.

McKiernan

S.M.

, Hagan

, Curry

Distinct MHC class I and II alleles are associated with hepatitis C viral clearance, originating from a single source. Hepatology. 2004; 40(1): 108–14.

295.

Yee

L.J.

Host genetic determinants in hepatitis C virus infection. Genes Immun. 2004; 5(4): 237–45.

296.

Hraber

, Kuiken

, Yusim

Evidence for human leukocyte antigen heterozygote advantage against hepatitis C virus infection. Hepatology. 2007; 46(6): 1713–21.

297.

Kuniholm

M.H.

, Kovacs

, Gao

Specific human leukocyte antigen class I and II alleles associated with hepatitis C virus viremia. Hepatology. 2010; 51(5): 1514–22.

298.

Kuniholm

M.H.

, Gao

, Xue

The relation of HLA genotype to hepatitis C viral load and markers of liver fibrosis in HIV-infected and HIV-uninfected women. J Infect Dis. 2011; 203(12): 1807–14.

299.

Thio

C.L.

, Thomas

D.L.

, Goedert

J.J.

Racial differences in HLA class II associations with hepatitis C virus outcomes. The J Infect Dis. 2001; 184(1): 16–21.

300.

Fanning

L.J.

, Levis

, Kenny-Walsh

, Whelton

, O'Sullivan

, Shanahan

HLA class II genes determine the natural variance of hepatitis C viral load. Hepatology. 2001; 33(1): 224–30.

301.

Marangon

A.V.

, Moliterno

R.A.

, Sell

A.M.

Influence of HLA alleles in response to treatment with pegylated interferon-alpha and ribavirin in patients with chronic hepatitis C. Int J Immunogenet. 2012.

302.

Yosry

, Fouad

, Mahmoud

, El-Raziky

M.S.

, El-Hennawy

, Ghoneim

M.A.

The association of HLA class II DR B1 alleles with HCV infection in Egyptian children. Arab J Gastroenterol. 2011; 12(1): 25–8.

303.

Corghi

D.B.

, Goncales

N.S.

, Marques

S.B.

, Goncales

F.L.

Jr. . Distribution of the human leukocyte antigen class II alleles in Brazilian patients with chronic hepatitis C virus infection. Braz J Med Biol Res. 2008; 41(10): 884–9.

304.

R-B

, Hong

, Ding

W-L

. The association between the genetic polymorphism of HLA-DQA1, DQB1, and DRB1 and serum alanine aminotransferase levels in chronic hepatitis C in the Chinese population. J Gastroenterol Hepatol. 2008; 23(9): 1394–402.

305.

Hardie

RALM

, Bruneau

, Knight

Human leukocyte antigen-DQ alleles and haplotypes and their associations with resistance and susceptibility to HIV-1 infection. AIDS. 2008; 22(7): 807–16.

306.

Shankarkumar

, Pawar

, Ghosh

, Bajpai

, Pazare

Human leucocyte antigen class II DRB1 and DQB1 associations in human immunodeficiency virus-infected patients of Mumbai, India. Int J Immunogenet. 2010; 37(3): 199–204.

307.

Malhotra

, Holte

, Dutta

Role for HLA class II molecules in HIV-1 suppression and cellular immunity following antiretroviral treatment. J Clin Invest. 2001; 107(4): 505–17.

308.

Lacap

P.A.

, Huntington

J.D.

, Luo

Associations of human leukocyte antigen DRB with resistance or susceptibility to HIV-1 infection in the Pumwani Sex Worker Cohort. AIDS. 2008; 22(9): 1029–38.

309.

Ryan

E.J.

, Dring

, Ryan

C.M.

Variant in CD209 promoter is associated with severity of liver disease in chronic hepatitis C virus infection. Human Immunology. 2010; 71(8): 829–32.

310.

Selvaraj

, Alagarasu

, Swaminathan

, Harishankar

, Narendran

CD209 gene polymorphisms in South Indian HIV and HIV-TB patients. Infect Genet Evol. 2009; 9(2): 256–62.

311.

Martin

M.P.

, Lederman

M.M.

, Hutcheson

H.B.

Association of DC-SIGN promoter polymorphism with increased risk for parenteral, but not mucosal, acquisition of human immunodeficiency virus type 1 infection. J Virol. 2004; 78(24): 14053–6.

312.

Liu

, Hwangbo

, Holte

Analysis of genetic polymorphisms in CCR5, CCR2, stromal cell-derived factor-1, RANTES, and dendritic cell-specific intercellular adhesion molecule-3-grabbing nonintegrin in seronegative individuals repeatedly exposed to HIV-1. J Infect Dis. 2004; 190(6): 1055–8.

313.

Koizumi

, Kageyama

, Fujiyama

RANTES-28G delays and DC-SIGN-139C enhances AIDS progression in HIV type 1-infected Japanese hemophiliacs. AIDS Res Hum Retroviruses. 2007; 23(5): 713–9.

314.

Liang

C.C.

, Liu

C.H.

, Lin

Y.L.

, Liu

C.J.

, Chiang

B.L.

, Kao

J.H.

Functional impairment of dendritic cells in patients infected with hepatitis C virus genotype 1 who failed peginterferon plus ribavirin therapy. J Med Virol. 2011; 83(7): 1212–20.

315.

Itose

, Kanto

, Inoue

Involvement of dendritic cell frequency and function in virological relapse in pegylated interferon-alpha and ribavirin therapy for chronic hepatitis C patients. J Med Virol. 2007; 79(5): 511–21.

316.

Simone

, Tortorella

, Zaccaro

, Napoli

, Antonaci

Impairment of TLR7-dependent signaling in dendritic cells from chronic hepatitis C virus (HCV)-infected non-responders to interferon/ribavirin therapy. J Clin Immunol. 2010; 30(4): 556–65.

317.

Kanto

, Inoue

, Oze

Dynamics of regulatory T cells and plasmacytoid dendritic cells as immune markers for virological response in pegylated interferon-α and ribavirin therapy for chronic hepatitis C patients. J Gastroenterol. 2012; 47(2): 169–78.

Dendritic Cells in HIV-1 and HCV Infection: Can They Help Win the Battle?

Abstract

Keywords

Introduction

Do HIV-1 and HCV Infect DCs?

HIV-1

HCV

Role of DCs in Viral Dissemination

HIV-1

HCV

Impact of Chronic HIV-1 and HCV Infection on DCs

Molecular Basis of Virus-DC Interaction

Crosstalk between DCs and NK Cells

HIV-1

HCV

Modulation of the Immunological Synapse: Role in HIV-1 and HCV Pathogenesis

HIV-1

HCV

Immune Response in the Liver: Role of Hepatic Antigen Presenting Cells

Impact of Host Genetic Variations on DC Functions during HIV-1 and HCV Infection

Future of Anti-HCV Treatment with and without HIV-1 Co-Infection

Conclusions and Future Perspectives

Author Contributions

Funding

Competing Interests

Disclosures and Ethics

Footnotes

Abbreviations

References