Xenotropic murine leukemia virus-related virus (XMRV) was generated after a recombination event between two endogenous murine leukemia viruses during the production of a prostate cancer cell line. Although the associations of the XMRV infection with human diseases appear unlikely, the XMRV is a retrovirus of undefined pathogenic potential, able to replicate in human cells in vitro. Since recent studies using animal models for infection have yielded conflicting results, we set out an ex vivo model for XMRV infection of human tonsillar tissue to determine whether XMRV produced by 22Rv1 cells is able to replicate in human lymphoid organs. Tonsil blocks were infected and infection kinetics and its pathogenic effects were monitored
XMRV, though restricted by APOBEC, enters and integrates into the tissue cells. The infection did not result in changes of T or B-cells, immune activation, nor inflammatory chemokines. Infectious viruses could be recovered from supernatants of infected tonsils by reinfecting DERSE XMRV indicator cell line, although these supernatants could not establish a new infection in fresh tonsil culture, indicating that in our model, the viral replication is controlled by innate antiviral restriction factors.
Overall, the replication-competent retrovirus XMRV, present in a high number of laboratories, is able to infect human lymphoid tissue and produce infectious viruses, even though they were unable to establish a new infection in fresh tonsillar tissue. Hereby, laboratories working with cell lines producing XMRV should have knowledge and understanding of the potential biological biohazardous risks of this virus.
Citation: Curriu M, Carrillo J, Massanella M, Garcia E, Cunyat F, et al. (2012) Susceptibility of Human Lymphoid Tissue Cultured ex vivo to Xenotropic Murine Leukemia Virus-Related Virus (XMRV) Infection. PLoS ONE 7(5): e37415. doi:10.1371/journal.pone.0037415
Editor: William M. Switzer, Centers for Disease Control and Prevention, United States of America
Received: February 22, 2012; Accepted: April 19, 2012; Published: May 16, 2012
Copyright: © 2012 Curriu et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This work was supported by the Fundación para la Investigación en Urología with a “Rafael Mollá y Rodrigo” scholarship and the “ayuda de investigación Pedro Cifuentes Díaz”. C. Cabrera and JB are researchers from Fundació Institut de Recerca en Ciències de la Salut Germans Trias i Pujol supported by the Health Department of the Catalan Government (Generalitat de Catalunya). MC is supported by a Spanish AIDS network “Red Temática Cooperativa de Investigación en SIDA” contract. FC is supported by the Fondo de. Investigación Sanitaria project 07/0418 and JC by the Sara Borrell postdoctoral program. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Xenotropic murine leukemia virus-related virus (XMRV) was initially identified in some prostate cancer tissues  and while several studies confirmed the presence of the virus in human prostate cancer cells with similar –, or lower prevalence –, other authors have reported no evidence of the virus in patient samples –. Later, this retrovirus was also detected in blood samples of a high proportion of individuals with chronic fatigue syndrome (CFS) , in the respiratory tract of patients with or without a respiratory tract infection , and a similar polytropic murine leukemia viruses (MLV) was found even in a high proportion of CFS cases . Nevertheless, several subsequent studies failed to identify XMRV in CFS patients or healthy donors –, and even blood samples from CFS patients previously reported to contain XMRV sequences were retested and were identified as XMRV negative , , . These data have resulted in the retraction of Lombardi et al. and Lo et al. papers –.
In order to explain the positive results, several studies suggested that the detection of XMRV sequences in human samples was a result of contamination of laboratory reagents with mouse DNA –, with DNA from the chronically infected DU145 cell line ,  or with a XMRV plasmid DNA . Finally, the assertion that XMRV is circulating in human population has been challenged by the report showing that XMRV was generated by a recombination event between two endogenous MLVs during in vivo tumor passaging in mice , which yielded the popular prostate cancer cell line 22Rv1 .
Figure 1. Detection of proviral XMRV DNA in human lymphoid tissue.
DNA was amplified by a single-round conventional PCR using a XMRV gag specific primer set and the PCR fragments were analysed on a 2% agarose-gel. A) XMRV-gag fragments in isolated tissue cells at the last day of the experiment in presence or absence of the antiretroviral inhibitors AZT and RAL. B) Proviral DNA content in cells migrating out of the tissue at different time points over the culture in absence or presence of AZT or RAL. PCR results from a representative experiment are shown.doi:10.1371/journal.pone.0037415.g001
Figure 2. Quantitative time course of XMRV gag sequences of ex vivo infected tonsillar tissue.
Isolated DNA was amplified by quantitative real-time PCR and the absolute XMRV copy numbers were obtained by normalizing the results with the values obtained with the single copy CCR5 gene in each sample. Each sample was run in duplicate. A) Absolute XMRV DNA content in tissue cells, after 22 days of infection, in the presence or absence of two antiretroviral drugs, AZT and RAL. B) XMRV DNA content in cells migrating out of the tissue collected from days 2 to 22 post-infection in the presence or absence of the indicated inhibitors.doi:10.1371/journal.pone.0037415.g002
Figure 3. XMRV RNA released by ex vivo human lymphoid tissue infected with 22Rv1 supernatant.
Blocks of tonsillar tissues were infected ex vivo with XMRV from 22Rv1 cells supernatant. Culture medium bathing the tissue blocks was changed every 3–4 days and analysed for the presence of XMRV RNA using a quantitative real-time RT-PCR. A) Cumulative amount of XMRV RNA released between days 9 and 22 post-inoculation in infected cultures in the presence or absence of the antiviral drugs AZT and RAL. The graph represents the viral RNA content in two donors (mean ± SEM). B) Kinetics of XMRV RNA released by infected tonsillar tissue and the effect of the addition of antiviral drugs to the culture.doi:10.1371/journal.pone.0037415.g003
Figure 4. Hypermutation of XMRV in infected human lymphoid tissue.
DNA from tonsillar tissue infected with XMRV was amplified, cloned and sequenced. A) Graphic representation of the changes (compared to XMRV VP42) presents in the XMRV gag region. The mutations presents in clones from 5 different donors are shown. Each mutation is denoted by a vertical line marked onto a single horizontal line representing the entire amplicon, color coded with respect to dinucleotide context: GG→AG (red). GA→AA (cyan), GC→AC (green), GT→AT (magenta), and non G→A (black). Analysis was performed using the HYPERMUT program . B) Preferences of nucleotide substitutions from all the obtained sequences, “n” denotes the total number of sequenced base pairs. C) Summary of the observed changes at the different dinucleotide context. “n” denotes the number of mutations; aPercentage of the total number of changes; bPercentage of the number of G-to-A changes.doi:10.1371/journal.pone.0037415.g004
Figure 5. Lymphocyte populations in uninfected and XMRV infected lymphoid tissue.
Tissue cells at day 9 post-infection were isolated, stained with monoclonal antibodies and analyzed using flow cytometry. Percentages of T (CD4+ and CD8+) and B cells in uninfected (XMRV−) and XMRV infected (XMRV+) tissues are shown. Data are means ± SEM from 5 independent infected tonsils.doi:10.1371/journal.pone.0037415.g005
Figure 6. Chemokine production of tonsillar tissues infected ex vivo with XMRV.
Tonsillar tissue was infected with XMRV and chemokine concentrations were measured using Cytometric Bead Array (CBA) in samples of culture medium collected at days 2, 5, 9, 13, 16 and 22. Data are presented as cumulative amount of released chemokines over the 22 days of culture in the absence or presence of AZT and RAL. Two separate experiments using two donors were carried out. Data presented are means ±SEM.doi:10.1371/journal.pone.0037415.g006
Figure 7. GFP-expression in DERSE XMRV indicator cells infected with tonsil supernatants.
DERSE XMRV indicator cells were infected with tonsil supernatants harvested at day 16 and 22 post-infection (donor 402, see Figure 3B) and with a XMRV stock (22Rv1 supernatant) as positive control. A) DERSE-GFP positive cells were visualized by conventional phase contrast microscopy and fluorescence microscopy. Phase contrast image (left panel), GFP fluorescence image (central panel) and GFP/phase contrast merge image (right panel). Data are representative of two independent experiments. B) Quantitative assessment of DERSE GFP-positive cells. After 7 and 10 days post-infection (D7 p.i. and D10 p.i.) DERSE infected cells were harvested and the percentage of GFP-expressing cells was analyzed by FACS analysis.doi:10.1371/journal.pone.0037415.g007
Figure 8. Re-infection of human lymphoid tissue with tonsil supernatants.
New histocultures from two different donors were prepared and infected at day 0 and 1 with a XMRV stock (22Rv1 supernatant) and supernatants harvested at day 16 and 22 post-infection (donor 402, Figure 3B). The positive control (22Rv1 supernatant) was cultured in the presence or absence of AZT. A) Proviral XMRV DNA analyzed by quantitative real-time PCR in tissue cells isolated after 28 days post-reinfection. Each sample was run in duplicate. B) Absolute proviral XMRV DNA content in cells migrating out of the tissue collected from days 7 to 28 post-reinfection. C) Kinetics of XMRV RNA released by lymphoid tissue into the medium analyzed by real-time qRT-PCR.doi:10.1371/journal.pone.0037415.g008
The 22Rv1 (ATCC CRL-2505) cell line was established from human prostate tumor explants after serially passing through athymic nude mice around 1991 – and has been widely used in laboratory experiments in prostate cancer research with over 198 citations in PubMed. Electron microscopic analysis of culture medium from this cell line revealed the presence of gammaretrovirus-like particles, further identified as a xenotropic murine leukemia virus-related virus (XMRV) showing multiple integrated copies and a high-level of viral production .
Despite the discovery of the origin of the virus and the accumulation of data showing that the virus is not present in the general human population, XMRV is a novel replication-competent virus and could be a potential human pathogen since it has been shown to successfully infect many human cell types in vitro , ,  including PBMCs and neuronal cells , , . Indeed, contamination of vertebrate cell lines with retroviruses has been widely described, being gammaretroviruses the most frequent contaminants –. About 60 copies of MLV sequences are present as endogenous proviruses in mouse genomes  from which up to 15 copies are related to infectious xenotropic murine leukemia viruses (XMLV) . The XMLV are type C retroviruses from mouse which can infect human or other foreign species – and have been identified in human cultures derived after xenografting immune compromised mice –. Recently, the presence of several MLV strains in over one fourth of xenograft cell lines has been documented , some of them releasing large number of infectious virions. This is the case of 22Rv1 cells, a high-titer XMRV producing cell line which should be carefully considered from the standpoint of possible horizontal spread to other human cells and biohazard of unknown potential to laboratory personnel . Regarding the virus transmission to other cell lines, two cell lines that have become infected with XMRV in the laboratory by a contamination with the 22Rv1cell line have already been reported, confirming the highly infectious nature of this virus , . Concerning the potential biohazards to laboratory personnel involved in cell culture facilities, it is important to explore XMRV infectivity and replication capacity in humans.
The infectivity of XMRV in humans may be strongly limited by innate host restriction factors such the APOBEC (apolipoprotein B mRNA-editing catalytic polypeptide) family, which play an important role in viral tropism, establishment of viral infections in vivo and successful spread of viruses. The family of APOBEC proteins, including APOBEC 3G and APOBEC 3F, have been implicated in the inhibition of a variety of retroviruses (HIV, SIV, HTLV and MLV) – and retrotransposons , . These proteins are cytidine deaminases, which when incorporated in viral particles alter the nascent retroviral DNA leading to massive G-to-A hypermutation of the viral genome , . In the case of XMRV, it has been shown that its replication is highly sensitive to APOBEC proteins and tetherin , , –. XMRV was hypermutated in A3G/A3F-expressing cell lines and in cultured human PBMCs, where replication was potently inhibited , . However, despite these observed in vitro restrictions, infectious XMRV was recovered from infected PBMCs when cocultured with a permissive cell line, suggesting that even if PBMCs do not support a productive infection, they may potentially act as a source of infectious XMRV in vivo , .
In the absence of any known human infection, information about the infectivity and replication capacity in humans is needed. Until now, animal models have been used for the study of the natural history of XMRV infection, although the infection of two non-human primate species has yielded conflicting results , . Organ cultures provide a versatile experimental system for studying the primary events surrounding virus transmission and the initiation of viral infections in human cells. It has been shown that human lymphoid tissue cultured ex vivo is a suitable model for HIV and HHV-6 pathogenesis –. In this system, HIV-1 infection results in cell activation and massive CD4+ T-cell depletion
The present study focuses on the characterization of infection of XMRV derived from the 22Rv1 cell line in lymphoid tissue ex vivo. We found that XMRV could infect human lymphoid tissue and infectious viruses were recovered capable to infect a DERSE XMRV indicator cell line, despite viral genomes were highly edited by APOBEC. However, the amount of virus released into the culture supernatant was not sufficient to establish a new infection in lymphoid tissue. The infection appears to have no pathogenic effects in lymphocytic populations or in the level of inflammatory chemokines, nonetheless, laboratories working with cell lines producing XMRV should have knowledge and understanding of the potential biological biohazardous risks of this virus.
Materials and Methods
Cells, viruses and antiviral agents
22Rv1 cells were obtained from the American Type Culture Collection (ATCC) and Detectors of Exogenous Retroviral Sequence Elements (DERSE) XMRV indicator cell line was kindly provided by Dr. Vineet N. KewalRamani (National Cancer Institute, Frederick, Maryland, USA). Both cell lines were maintained in RPMI 1640 medium with 10% FBS (Invitrogen, Spain). Cell-free XMRV was harvested from 22Rv1 supernatant, clarified by centrifugation; aliquots were stored at −80°C until used. Zidovudine (AZT) was purchased from Sigma-Aldrich (Spain) and Raltegravir (RAL) was obtained through the AIDS Research and Reference Reagent Program, Division of AIDS, NIAID, NIH; from Merck & Company, Inc.
XMRV infection of human lymphoid tissue ex vivo
Human tonsils were obtained from patients undergoing therapeutic tonsillectomies. All procedures followed the Helsinki Declaration in 1975, as revised in 1983, and were approved by the Ethics committee of the Hospital Germans Trias i Pujol. All individuals provided their written informed consent. The specimens were dissected into ~2–3 mm3 blocks, and cultured in RPMI 1640 medium supplemented with 15% fetal bovine serum, 1 mM sodium pyruvate (Invitrogen Life Technologies, Spain), 0.1 mM minimal essential medium with nonessential amino acids (Invitrogen) and a mixture of antibiotics on top of collagen sponge gels at the medium-air interface as previously described .. Nine individual blocks were placed on the gelfoam in a well of a six-well plate. Lymphoid tissue blocks were left uninfected or were infected with 5 µL of XMRV stock (4×108 RNA copies/mL) for each tissue block. Cultures were conducted in the absence or the presence of reverse transcriptase or integrase inhibitors, AZT (10 µg/mL) or RAL (5 µg/mL), respectively. Fresh drug was added at every medium change. Each experimental condition was composed of three wells for a total of 27 blocks whose culture media were pooled. Culture medium was harvested every 3–4 days, centrifuged and both, the pellets with the cells migrating out of the tissue, and the clarified supernatant were frozen at −80C until use. On days 14 to 22 after infection, cells were mechanically isolated from uninfected and infected tissue blocks and immunophenotyped. Cell Pellets were also stored at −80°C for further analyses.
XMRV DNA detection
Viral infection was evaluated at different time points in the cells migrating out of the tissue and in tissue cells at the end of the culture by analyzing the presence of viral DNA by conventional PCR. DNA was isolated using QIAamp DNA Blood kit (Qiagen, Spain) according to the manufacturer's instructions, and gag gene was amplified as previously described . Briefly, PCR was conducted with 5 µL of extracted DNA and the primers 419F and 1154R using Accuprime Taq DNA Polymerase (Invitrogen, Spain). The cycles were 10 min at 94°C (30 sec at 94°C, 30 sec at 57°C, 1 min 68°C)×40 cycles and 10 min at 68°C. Then, samples were electrophoresed in 2% agarose gels containing SYBR safe DNA in TAE buffer.
Quantitative Real-Time PCR
To quantify the absolute XMRV DNA copy numbers, standard plasmids for XMRV-gag and for the single-copy CCR5 gene were used. Both plasmids were constructed by conventional PCR using AmpliTaq High Fidelity (Invitrogen, Spain) and the following primers: Q445F and Q528R previously described for the detection of XMRV gag  and CCR5-576F (5′-TCATTACACCTGCAGCTCTCATTT-3′) and CCR5-726R (5′- ACACCGAAGCAGAGTTTTTAGGAT-3′) for CCR5 detection. The two PCR products purified with QIAquick PCR Purification Kit (Qiagen, Spain) were cloned into a PCR-Script Amp Cloning Kit (Agilent, Spain) according to the manufacturer's instructions. The plasmids were purified by standard methods, their concentrations were measured using a fluorometer and the corresponding copy numbers were calculated. Quantitative real-time PCR was performed with DNA isolated from the cells migrating out the tissue at different time-point during the culture and in tissue cells at the end of the culture in duplicate, using a TaqMan Universal Master Mix (Applied Biosystems, Spain), the primers described above and the probes: F480PRO; (5′-FAM-ACAGAGACACTTCCCGCCCCCG-MGBNFQ-3′)and CCR5-661T (5′-VIC-CTGGTCCTGCCGCTGCTTGTCA-TAMRA-3′) to detect XMRV gag and CCR5, respectively. A ten-fold serial dilution of the two standard plasmids, ranging from 1×1010 to 1×10−1 copies/reaction was used in duplicate to construct standard curves. All real-time PCR reactions were performed on a ABI Prism 7000 (Applied Biosystems, Spain).
Quantification of viral RNA released
Quantitative measurements of XMRV viral RNA in culture supernatants were done using a quantitative real-time RT-PCR assay. Total RNA was extracted from 280 µL of culture supernatant at different time points during the culture (QIAamp Viral RNA kit, Qiagen, Spain) and one-step quantitative reverse transcription PCR was performed using the Ag-path-ID One-Step RT-PCR Kit from Ambion (Applied Biosystems, Spain) using the primers, probes and standard curves described above.
G-to-A hypermutation of XMRV proviruses in infected tissue cells
PCR products obtained by conventional PCR from tissue cells (see above) were cloned using the PCR-Script Amp Cloning Kit. Over 10–30 colonies were selected for each product and sequenced using the Big-Dye Terminator Cycle Sequencing and the ABI 3100 sequence analyzer (Applied Biosystems, Spain). All sequences were assembled, aligned and edited using the Sequencher v.4.2 and GeneDoc v.2.6.001 software. The alignments were uploaded to the Hypermut tool on the Los Alamos National Laboratories website (http://www.hiv.lanl.gov/content/sequence/HYPERMUT/hypermut.html) to identify hypermutated sequences .
Infectivity of newly produced viruses by infected tonsils
To analyze infectivity of supernatants from XMRV-infected tonsils we used two different approaches. First, infection of the DERSE XMRV indicator cell line was performed. The development of DERSE cells involved the transfection of LNCaPs cells with a MLV reporter vector encoding puromycin resistance and a CMV enhancer/promoter driven GFP reporter gene whose transcription was antisense to the vector mRNA (KewalRamani VN, unpublished data). DERSE XMRV indicator cells were plated at a density of 40,000 cells/well in 48-well plates and allowed to grow overnight. Next day, the cells were infected with culture supernatant (50 µL) of previous tonsils infected and harvested at days 16 and 22 post-infection (donor 402). As a positive control we infected one well with the 22Rv1 supernatant stock. The culture was splitted at days 3, and 7 and maintained for 10 days. The percentage of GFP-expressing cells was evaluated by fluorescence microscopy and flow cytometry. In addition, new tonsils histocultures were re-infected with supernatant harvested at day 16 and 22 (donor 401 and 402) from previous histocultures infections. The infection was done at day 0 as described above although here the tissue was re-infected with the same amount of virus at day 1 of culture. The culture was maintained 28 days and culture medium, cells migrating out of the tissue and tissue cells were harvested as previously described.
Immunophenotypic characterization of tissue lymphocytes
Single cell suspensions were prepared as described above. Tissue lymphocytes at the end of the culture were immunophenotyped using monoclonal antibodies against the following surface antigens: CD3, CD4, CD8, CD45RO, CD38 and HLA-DR for the analysis of T cell, and CD19, IgD, CD38, CD27, from Becton Dickinson, Barcelona, Spain) and CD10 for B cells (from eBioscience, Barcelona, Spain). Multicolor analysis was performed with a LSRII flow cytometer (Becton Dickinson). Data were acquired with the BD FACSDiva software and analyzed with Flow Jo software.
Flow cytometric analysis of chemokines
Culture supernatants clarified by centrifugation and collected at different time points during culture were assayed using a Cytometric Bead Array kit (CBA, BD Biosciences, Spain). Chemokines (CXCL8/IL-8, RANTES, CXCL9/MIG, CCL2/MCP-1, and CXCL10/IP-10) were measured using the Human Chemokine kit according to the manufacturer's instructions using a LSRII flow cytometer (Becton Dickinson).
XMRV infection of human lymphoid tissue
To evaluate the ability of XMRV to infect human lymphoid tissue, infectious XMRV harvested from prostate carcinoma cell line 22Rv1 was used to infect tonsillar explants ex vivo. After 14 days post-infection, we analyzed the presence of XMRV gag proviral DNA in tissue blocks. Cells were mechanically isolated from uninfected and infected tissue and the presence of XMRV gag proviral DNA was clearly observed in infected tissue cells by conventional PCR at the end of each experiment (Figure 1A). The specificity of the infection was evaluated using AZT and RAL, two antiretroviral drugs known to inhibit XMRV reverse transcriptase (RT) and integrase, respectively , . Both drugs completely inhibited XMRV DNA detection in tissue cells, indicating that infection is the result of specific reverse transcription and integration processes (Figure 1A). To assess the kinetics of the infection we quantified the XMRV proviral DNA in cells migrating out the tissue, which were collected every 3–4 days. After 3 days of culture, migrating cells were already XMRV positive and remained positive until the last day tested (Figure 1B). The RT inhibitor AZT markedly inhibited the presence of XMRV proviral DNA in all time points. Conversely, modest effects were observed after 7 or 14 days in the presence of the integrase inhibitor RAL (Figure 1B). Cells from the mock-infected tissue were negative in all cases.
Increase in proviral XMRV DNA content during the culture of human lymphoid tissue
Once we confirmed the entry and the reverse transcription of XMRV in the human lymphoid tissue, we accurately evaluated the level of the infection by setting up a quantitative real-time PCR to measure the absolute XMRV DNA content. Total XMRV gag copies per 1×106 cells were obtained for several tissues by CCR5 normalization after 22 days of infection (Figure 2). A clear increase in the amount of proviral DNA present in tissue cells was observed when comparing with the histocultures infected in the presence of antiretroviral drugs. The treatment with AZT and RAL resulted in almost complete inhibition (>97%) at most time points and donors tested (Figure 2A). In migrating cells, the increase in the infection was detected after 9–10 days of culture, although the proviral DNA content underwent a significant increase at later points (after 16 days post-infection, Figure 2B). The presence of AZT in the culture reduced proviral DNA level to negative values from day 3 to the end of cultures. However, in the presence of RAL, proviral DNA values were comparable to the infected tissue without drug and remained stable until day 7–13, declining at the last days of culture (Figure 2B). This different behaviour in the inhibition between both drugs could be explained by the fact that our PCR system detected not only the integrated DNA, but also unintegrated DNA. AZT would totally block viral DNA synthesis, resulting in decrease of both total and integrated DNA. On the contrary, when an integration inhibitor like RAL is used, unintegrated viral DNA accumulates in the nuclei in the form of 1-LTR and 2-LTR circles . These episomal forms may explain the detection of XMRV DNA at an almost constant value over time in our infected tissue in the presence of RAL.
XMRV RNA detection in the supernatant of infected histocultures
The observed increase in viral DNA content in both, tissue and migrating cells, indicated that XMRV might establish a productive infection in our histoculture model. To evaluate this possibility, XMRV RNA released into the medium, starting on day 5 post-infection, was quantified in culture supernatants by using real-time qRT-PCR. The cumulative production in the infected cultures from day 9 to day 22 post-infection is shown in Figure 3A. XMRV RNA was mainly detected in infected tissues that were cultured without antiviral drugs. The total production of viral RNA in AZT and RAL containing cultures constituted only the 8 and 4%, respectively of the infected tissues without drug (Figure 3A). The evaluation of replication kinetics revealed a decrease in RNA viral levels up to day 9 in cultures with or without drug, representing the washing out of the starting viral inoculums (Figure 3B). Thereafter, RNA virus release experienced a continuous increase over time in infected tissue without drug from day 9 to the last day of culture, reaching levels up to 2×106 copies/mL after 22 days of culture. This increase in RNA virus release, ranging from 16- to 21-fold in the different tested donors, was completely blocked by AZT or RAL (Figure 3B). These findings could indicate that XMRV production, which is sensitive to RT and integrase inhibitors, occurs in tonsillar tissue.
Host restriction of XMRV in human lymphoid tissue
A severe restriction in the spreading of the XMRV infection has been shown in PHA-activated human PBMCs . Since human lymphocytes express restriction factors, such as APOBEC 3G and 3F, ,  we sought to determine whether these factors impacted on XMRV replication in tonsils. DNA from infected tissue cells at the last day of the experiment was isolated and a 731-base pair fragment of the XMRV gag region was amplified. The PCR products were cloned and their DNA sequences were compared to the XMRV VP42 consensus. A total of 80 clones derived from 5 different donors were analyzed (Figure 4A). An initial analysis revealed that 46 sequences (57.5%) had mutations, although only 32 (40%) of them harbored more than one mutation. To identify the hypermutated sequences we used the LANL Hypermut 2.0 program , using a p-value<0.05. Compared to XMRV VP42, a total of 15 (18.8%) sequences were identified as hypermutated, with a range of 0 to 31.2% among different donors. In total, 180 changes were detected with a mutation frequency of 3×10−3/nt (180 mutations for 58480 nucleotides sequenced) of which 142 were G-to-A changes (Figure 4B). Substitutions in the GG dinucleotide context (GG-to-AG), which is the specific target site for APOBEC 3G , , were more prevalent (76%) than in the APOBEC 3F-preferred context (GA-to-AA) (20%), suggesting that XMRV in our ex vivo infection is mainly restricted by APOBEC 3G (Figure 4). At the amino acid level, mutations caused both, changes in the amino acid sequence and introduction of stop codons.
Pathogenic effects of XMRV infection
To further characterize the XMRV infection in tonsillar tissue, we investigated possible pathogenic effects. It has been shown that HIV-1 severely depletes CD4+ T-cells in ex vivo infected human lymphoid tissue , , with a depletion of 77 and 97% of CD4+ T-cells relative to uninfected samples after 8 and 13 days post-infection, respectively . Therefore, we addressed whether XMRV replication may alter tissue lymphocytes. Despite the apparent infection of the tissue, we did not observed changes in the percentage of the main lymphocyte populations after 9 days of infection (Figure 5). XMRV infection did not modify the percentage of CD3+ T-cells (63±11% and 64±8% in XMRV− and XMRV+ tissue, respectively), nor CD4+ T-cells (47±7% vs 48±5%), nor CD8+ T-cells (20±12% vs 19±11%). The percentages of B cells were also similar between both tissues, CD19+ cells (29±16% vs 27±14%) (Figure 5). A deeper analysis of T-cell subsets showed that XMRV infection did not modify the naïve/memory cell ratio, in both T and B cells, nor immune activation markers, evaluated by the expression of CD38 and HLA-DR in both CD4+ and CD8+ T-cells (data no shown). None of these parameters was modified after 28 days in culture (data no shown).
Release of different chemokines upon XMRV tissue infection
In human lymphoid tissue infected with other viruses such as HIV and HHV-6 a modulation in the chemokine secretion by viral replication has been documented , , . To address this possibility, five chemokines from a designed Human Chemokine kit, some of them previously described to be altered in patients with CFS ,  were measured by using a quantitative cytometric bead array on the supernatants collected during the course of 22 days of viral infection The total production of those chemokines did not significantly change by XMRV infection in the absence or presence of antiviral drugs (Figure 6).
Recovery of replication-competent XMRV from supernatants of infected tonsils
The increase in DNA and viral RNA together with the presence of hypermutated sequences suggests an active replication. To evaluate if the supernatant of infected tonsils histocultures contained replication-competent virus, we performed a viral infectivity assay using DERSE XMRV indicator cells, which were infected with those supernatants. The indicator cell line DERSE XMRV will only produce GFP following infection with a replication-competent virus since the gfp gene is functionally reconstituted upon reverse transcription. DERSE cells were infected with 50 µL of supernatants harvested at day 16 and 22 (donor 402, Figure 3B) which contained 23,000 and 99,000 copies of XMRV RNA, respectively and with XMRV from 22Rv1 supernatant stock (40,000 copies of RNA) and the GFP expression was monitored by fluorescence microscopy every 2–3 days of infection. GFP+ cells were detected in the control culture (infected with 22Rv1 supernatant stock) as early as 3 days (data not shown) and a high number of cells were positive at day 7 post-infection (Figure 7A). At this time, GFP expression was also observed when cells were infected with the supernatants of infected tonsil, (Figure 7A middle and lower panels). No GFP expression was detected in mock-infected cells. To quantify the percentage of cells infected with each supernatant, DERSE cells were harvested and analyzed by flow cytometry at different days after infection. At 7 days post-infection a high number of GFP+ cells (28%) were detected when a 22Rv1 supernatant stock was used (Figure 7B). In the infections with the supernatants from day 16 and 22, and in agreement with the data observed by microscopy, a lower number of GFP+ cells were detected (4% and 7%, respectively), although the levels were significantly higher than those observed in uninfected wells (Figure 7B) at day 7. Following culture passage, an increase in the number of GFP+ cells was observed in all the infections, reaching similar values in the infections with both supernatant than in the infection with the 22Rv1 stock (21% and 27% of GFP+ cells with supernatants from day 16 and 22, respectively, and 29% of GFP+ cells with 22Rv1 supernatant. Figure 7B). The results from this viral infectivity assay suggested that XMRV viral particles, which were able to replicate and spread were presents in the tonsillar supernatants.
Furthermore, we analyze the ability of tonsillar supernatants to re-infect a new histoculture. In order to maximize the infection, tissue from two different donors was infected at day 0 and re-infected with the same amount of virus at day 1. We use each time 45 µL (5 µL for each tissue block) of XMRV 22Rv1 stock (4×108 copies/mL), donor 402 supernatant day 16 (4.7×105 copies/mL) and donor 402 supernatant day 22 (2×106 copies/mL) (see Figure 3A). After 28 days of infection we observed a very large number of copies of proviral DNA in tissue cells infected with 22Rv1 supernatant and almost a total inhibition with AZT. However, none of the tonsil supernatants used to re-infect the tissue was able to infect this new tissue and only a residual amount of proviral DNA (even lower than that detected in the infection of 22Rv1+AZT) was observed, mainly in the supernatant from day 22 (Figure 8A). Consistent with the lack of detection of proviral DNA in tissue cells, we found only a residual level of both, proviral DNA in cells migrating out of the tissue (Figure 8B) and XMRV RNA released into the medium (Figure 8C).
During the last year an enormous amount of data about the origin and the prevalence of XMRV have indicated that this virus has a recombinant origin and it is not circulating in the human population –, –, –, although many questions about the biology and physiopathology of this virus remain still unclear.
Despite all these data and considering, i) the susceptibility of humans cells to the XMRV infection , , , ii) the contradictory data on experimental infection of macaques by XMRV , , iii) the high-titer production of XMRV by the 22Rv1 cell line, widely used in laboratory, and iv) the existence of XMRV/human contacts in laboratory personnel involved in cell culture facilities, it could be relevant to develop new experimental models for the study of XMRV pathogenesis in humans alternative to the use of non-human primates.
The main objective of the present study was to investigate whether the human lymphoid tissue might be a target for XMRV derived from 22Rv1 supernatant. We used histocultures of human tonsillar tissues that have been reported as a useful model for studying various aspects of the pathogenesis of other viruses , , . The ex vivo infection with XMRV allowed us to assess the replication of the virus, in addition to the pathogenic effects of this infection in human lymphoid tissue.
Tonsillar tissue after 14–22 days of infection become efficiently and specifically infected by XMRV. In contrast to previously described findings using in vitro infected PBMCs, the proviral copy numbers in our ex vivo infected histoculture increased overtime from day 2 to day 22 which could indicate that new target cells become infected throughout the culture. This increase in the proviral DNA content was concomitant to the increase in XMRV RNA released into the culture medium, suggesting that this XMRV RNA is associated with infectious particles that may lead to the spread of the infection. When the presence of infectious viral particles in the supernatants of infected tonsils was evaluated, we observed that we could recover replication-competent XMRV from these supernatants by infecting the indicator DERSE XMRV cell line. In contrast, those supernatants were unable to establish an infection in fresh lymphoid tissue, suggesting that with the passage of the virus through several rounds of infection, the innate antiviral restriction factors may abrogate its infectivity. Nevertheless, it should be noted that these supernatants have a much lower amount (2 to 3 log-copies of RNA/mL less) that the 22Rv1 supernatant used as a positive control of infection. Indeed, a high viral titer is required to establish an infection in human PBMCs , , so it is possible that viruses released by tonsils, although infectious in the DERSE assay, did not reach a sufficient titer to establish a new histoculture infection. In addition, the increase in proviral copy numbers, both in the tissue and the migrating cells, could be fully explained by cell divisions of infected cells, which in turn would lead to an increase in the level of released XMRV RNA.
Although the absolute levels of XMRV RNA released varied from donor to donor, the replication was similar to those observed in tonsillar tissue infected with some strains of HIV (R5 strains) (ranging between 2 and 5×106 RNA copies/mL) , but lower than viral production of more pathogenic strains of HIV (×4 strains), which range from 15 to 60×106 RNA copies/mL . However, for HIV has never been reported whether this amount of virus produced is sufficient to establish a new productive infection in a new histoculture.
Our observation that we could not establish a new infection in tonsillar tissue may indicate that, in ex vivo infected human lymphoid tissue, the virus is restricted by innate host restriction factors such the APOBEC family, since hypermutation, the introduction of excessive G-to-A substitutions by those host proteins that impair the viral replication, has also been observed in our experimental model. The sequence analysis of our clones showed that 19% of the sequences were hypermutated. This percentage, although lower than the 77 and 65% of hypermutated sequences found with the infection of two APOBEC 3G/3F positive cell lines (CEM and H9, respectively) , is similar with the level of hypermutagenesis described in the infection of PHA-stimulated PBMCs . In addition, the mutation frequencies obtained from our sequences (3×10−3/nt) were higher than those found in 22Rv1 proviral DNA (4.9×10−4/nt) or with the infection of an APOBEC 3G/3F negative cell (CEM-SS) (8.4×10−4/nt), although they were similar to those found in the infection of H9 cells (6.6×10−3/nt) . Moreover, although G-to-A mutations can occur in one of four different dinucleotide contexts (GG, GA, GC or GT), APOBEC 3G induces twice as many GG-to-AG as GA-to-AA changes , while APOBEC 3F primarily induce GA-to-AA . In tissue, most of the G-to-A changes occurred in a GG dinucleotide context. Overall, our data indicate that XMRV infection would be restricted, mainly by APOBEC 3G, as described in in vitro infected PBMCs or human cell lines. Nonetheless, in lymphoid tissue, the virus could somehow be able to evade or overcome these restriction factors, as a low amount of infectious virus is released. There are various non-excluding explanations for this observation. The most obvious conjecture could be that the level of APOBEC 3G is lower in lymphoid tissue than in peripheral PBMCs and not enough to block virus replication. However, all APOBEC family members are expressed widely in hematopoietic cell populations and in tissues, particularly in tonsils . Secondly, despite the fact that our data show that mechanically isolated lymphocytes from tissue and migrating cells are XMRV DNA+, the cell population responsible for the viral production remains unknown. In our histocultures, XMRV could infect other cell types that do not express these restriction factors, being a non-lymphoid cell the major viral target as it was shown in prostate cancer tissues  or in tissues from experimentally infected monkeys . Further work is necessary to define the cellular population that would sustain this low viral production in ex vivo infected tonsils.
In ex vivo HIV infected tonsils, virus replication causes a profound depletion of the viral target cells (CD4+ T cells). In our histocultures, we did not observe changes in the percentages in any of the major lymphocyte populations or modifications in the release of inflammatory chemokines. Yet, in XMRV infected macaques the virus did not induce any lymphocyte depletion, rather there was an increase in the frequency of circulating B and NK cells in blood .
In conclusion, in the absence of any confirmed human XMRV infection and with the conflicting results of infection in animal models, which may not accurately mimic human XMRV infection, in our ex vivo cultured human lymphoid tissue, XMRV is able to infect tissue cells and produce infectious viruses, even though they were unable to establish a new infection in fresh tonsillar tissue. The XMRV replication is largely controlled by innate antiviral restriction factors and probably further contained by the adaptative immune response, although the long term presence of proviral DNA and viral RNA in the lymphoid tissue remains absolutely unknown. Hereby, laboratories working with XMRV producing cell lines should be aware of the potential biohazard risk of working with this replication-competent retrovirus.
We thank Dr. KyeongEun Lee and Dr. Vineet KewalRamani for providing us with the (DERSE) XMRV indicator cell line.
Conceived and designed the experiments: JA MB BC JB PW C. Cabrera. Performed the experiments: MC EG JC MM FC C. Cabrera RP. Analyzed the data: MC JB C. Cabrera. Contributed reagents/materials/analysis tools: PW C. Carrato. Wrote the paper: MC JB C. Cabrera.
- 1. Urisman A, Molinaro RJ, Fischer N, Plummer SJ, Casey G, et al. (2006) Identification of a novel Gammaretrovirus in prostate tumors of patients homozygous for R462Q RNASEL variant. PLoS Pathog 2: e25.
- 2. Danielson BP, Ayala GE, Kimata JT (2010) Detection of xenotropic murine leukemia virus-related virus in normal and tumor tissue of patients from the southern United States with prostate cancer is dependent on specific polymerase chain reaction conditions. J Infect Dis 202: 1470–1477.
- 3. Schlaberg R, Choe DJ, Brown KR, Thaker HM, Singh IR (2009) XMRV is present in malignant prostatic epithelium and is associated with prostate cancer, especially high-grade tumors. Proc Natl Acad Sci U S A 106: 16351–16356.
- 4. Kim S, Kim N, Dong B, Boren D, Lee SA, et al. (2008) Integration site preference of xenotropic murine leukemia virus-related virus, a new human retrovirus associated with prostate cancer. J Virol 82: 9964–9977.
- 5. Arnold RS, Makarova NV, Osunkoya AO, Suppiah S, Scott TA, et al. (2010) XMRV infection in patients with prostate cancer: novel serologic assay and correlation with PCR and FISH. Urology 75: 755–761.
- 6. Hong S, Klein EA, Das Gupta J, Hanke K, Weight CJ, et al. (2009) Fibrils of prostatic acid phosphatase fragments boost infections with XMRV (xenotropic murine leukemia virus-related virus), a human retrovirus associated with prostate cancer. J Virol 83: 6995–7003.
- 7. Dong B, Kim S, Hong S, Das Gupta J, Malathi K, et al. (2007) An infectious retrovirus susceptible to an IFN antiviral pathway from human prostate tumors. Proc Natl Acad Sci U S A 104: 1655–1660.
- 8. Fischer N, Hellwinkel O, Schulz C, Chun FK, Huland H, et al. (2008) Prevalence of human gammaretrovirus XMRV in sporadic prostate cancer. J Clin Virol 43: 277–283.
- 9. Switzer WM, Jia H, Zheng H, Tang S, Heneine W (2011) No association of xenotropic murine leukemia virus-related viruses with prostate cancer. PLoS One 6: e19065.
- 10. Verhaegh GW, de Jong AS, Smit FP, Jannink SA, Melchers WJ, et al. (2011) Prevalence of human xenotropic murine leukemia virus-related gammaretrovirus (XMRV) in Dutch prostate cancer patients. Prostate 71: 415–420.
- 11. Barnes E, Flanagan P, Brown A, Robinson N, Brown H, et al. (2010) Failure to detect xenotropic murine leukemia virus-related virus in blood of individuals at high risk of blood-borne viral infections. J Infect Dis 202: 1482–1485.
- 12. Hohn O, Krause H, Barbarotto P, Niederstadt L, Beimforde N, et al. (2009) Lack of evidence for xenotropic murine leukemia virus-related virus(XMRV) in German prostate cancer patients. Retrovirology 6: 92.
- 13. Sfanos KS, Sauvageot J, Fedor HL, Dick JD, De Marzo AM, et al. (2008) A molecular analysis of prokaryotic and viral DNA sequences in prostate tissue from patients with prostate cancer indicates the presence of multiple and diverse microorganisms. Prostate 68: 306–320.
- 14. Sabunciyan S, Mandelberg N, Rabkin CS, Yolken R, Viscidi R (2011) No difference in antibody titers against xenotropic MLV related virus in prostate cancer cases and cancer-free controls. Mol Cell Probes 25: 134–136.
- 15. Akgul B, Pfister D, Knuchel R, Heidenreich A, Wieland U, et al. (2011) No evidence for a role of xenotropic murine leukaemia virus-related virus and BK virus in prostate cancer of German patients. Med Microbiol Immunol.
- 16. Cool M, Bouchard N, Masse G, Laganiere B, Dumont A, et al. (2011) No detectable XMRV in subjects with chronic fatigue syndrome from Quebec. Virology.
- 17. Stieler K, Schindler S, Schlomm T, Hohn O, Bannert N, et al. (2011) No detection of XMRV in blood samples and tissue sections from prostate cancer patients in Northern Europe. PLoS One 6: e25592.
- 18. Martinez-Fierro ML, Leach RJ, Gomez-Guerra LS, Garza-Guajardo R, Johnson-Pais T, et al. (2010) Identification of viral infections in the prostate and evaluation of their association with cancer. BMC Cancer 10: 326.
- 19. Aloia AL, Sfanos KS, Isaacs WB, Zheng Q, Maldarelli F, et al. (2010) XMRV: a new virus in prostate cancer? Cancer Res 70: 10028–10033.
- 20. Lombardi VC, Ruscetti FW, Das Gupta J, Pfost MA, Hagen KS, et al. (2009) Detection of an infectious retrovirus, XMRV, in blood cells of patients with chronic fatigue syndrome. Science 326: 585–589.
- 21. Fischer N, Schulz C, Stieler K, Hohn O, Lange C, et al. (2010) Xenotropic murine leukemia virus-related gammaretrovirus in respiratory tract. Emerg Infect Dis 16: 1000–1002.
- 22. Lo SC, Pripuzova N, Li B, Komaroff AL, Hung GC, et al. (2010) Detection of MLV-related virus gene sequences in blood of patients with chronic fatigue syndrome and healthy blood donors. Proc Natl Acad Sci U S A 107: 15874–15879.
- 23. Erlwein O, Kaye S, McClure MO, Weber J, Wills G, et al. (2010) Failure to detect the novel retrovirus XMRV in chronic fatigue syndrome. PLoS One 5: e8519.
- 24. Groom HC, Boucherit VC, Makinson K, Randal E, Baptista S, et al. (2010) Absence of xenotropic murine leukaemia virus-related virus in UK patients with chronic fatigue syndrome. Retrovirology 7: 10.
- 25. Henrich TJ, Li JZ, Felsenstein D, Kotton CN, Plenge RM, et al. (2010) Xenotropic murine leukemia virus-related virus prevalence in patients with chronic fatigue syndrome or chronic immunomodulatory conditions. J Infect Dis 202: 1478–1481.
- 26. Switzer WM, Jia H, Hohn O, Zheng H, Tang S, et al. (2010) Absence of evidence of xenotropic murine leukemia virus-related virus infection in persons with chronic fatigue syndrome and healthy controls in the United States. Retrovirology 7: 57.
- 27. Shin CH, Bateman L, Schlaberg R, Bunker AM, Leonard CJ, et al. (2011) Absence of XMRV and other MLV-related viruses in patients with Chronic Fatigue Syndrome. J Virol.
- 28. Satterfield BC, Garcia RA, Jia H, Tang S, Zheng H, et al. (2011) Serologic and PCR testing of persons with chronic fatigue syndrome in the United States shows no association with xenotropic or polytropic murine leukemia virus-related viruses. Retrovirology 8: 12.
- 29. Hong P, Li J, Li Y (2010) Failure to detect Xenotropic murine leukaemia virus-related virus in Chinese patients with chronic fatigue syndrome. Virol J 7: 224.
- 30. Mi Z, Lu Y, Zhang S, An X, Wang X, et al. (2011) Absence of xenotropic murine leukemia virus-related virus in blood donors in China. Transfusion.
- 31. Knox K, Carrigan D, Simmons G, Teque F, Zhou Y, et al. (2011) No evidence of murine-like gammaretroviruses in CFS patients previously identified as XMRV-infected. Science 333: 94–97.
- 32. Alberts B (2011) Editorial Expression of Concern. Science.
- 33. Silverman RH, Das Gupta J, Lombardi VC, Ruscetti FW, Pfost MA, et al. (2011) Partial retraction. Detection of an infectious retrovirus, XMRV, in blood cells of patients with chronic fatigue syndrome. Science 334: 176.
- 34. Alberts B (2011) Retraction. Science 334: 1636.
- 35. Lo SC, Pripuzova N, Li B, Komaroff AL, Hung GC, et al. (2012) Retraction for Lo et al., Detection of MLV-related virus gene sequences in blood of patients with chronic fatigue syndrome and healthy blood donors. Proc Natl Acad Sci U S A 109: 346.
- 36. Hue S, Gray ER, Gall A, Katzourakis A, Tan CP, et al. (2010) Disease-associated XMRV sequences are consistent with laboratory contamination. Retrovirology 7: 111.
- 37. Oakes B, Tai AK, Cingoz O, Henefield MH, Levine S, et al. (2010) Contamination of human DNA samples with mouse DNA can lead to false detection of XMRV-like sequences. Retrovirology 7: 109.
- 38. Robinson MJ, Erlwein OW, Kaye S, Weber J, Cingoz O, et al. (2010) Mouse DNA contamination in human tissue tested for XMRV. Retrovirology 7: 108.
- 39. Sato E, Furuta RA, Miyazawa T (2010) An endogenous murine leukemia viral genome contaminant in a commercial RT-PCR kit is amplified using standard primers for XMRV. Retrovirology 7: 110.
- 40. Smith RA (2010) Contamination of clinical specimens with MLV-encoding nucleic acids: implications for XMRV and other candidate human retroviruses. Retrovirology 7: 112.
- 41. Katzourakis A, Hue S, Kellam P, Towers GJ (2011) Phylogenetic analysis of MLV sequences from longitudinally sampled Chronic Fatigue Syndrome patients suggests PCR contamination rather than viral evolution. J Virol.
- 42. Wolff D, Gerritzen A (2011) Presence of murine leukemia virus (MLV)-related virus gene sequences in a commercial RT-PCR reagent. Clin Lab 57: 631–634.
- 43. Erlwein O, Robinson MJ, Dustan S, Weber J, Kaye S, et al. (2011) DNA extraction columns contaminated with murine sequences. PLoS One 6: e23484.
- 44. Tuke PW, Tettmar KI, Tamuri A, Stoye JP, Tedder RS (2011) PCR master mixes harbour murine DNA sequences. Caveat emptor! PLoS One 6: e19953.
- 45. Garson JA, Kellam P, Towers GJ (2011) Analysis of XMRV integration sites from human prostate cancer tissues suggests PCR contamination rather than genuine human infection. Retrovirology 8: 13.
- 46. Rusmevichientong A, Das Gupta J, Elias PS, Silverman RH, Chow SA (2011) Analysis of single-nucleotide polymorphisms in patient-derived retrovirus integration sites reveals contamination from cell lines acutely infected by xenotropic murine leukemia virus-related virus. J Virol 85: 12830–12834.
- 47. Paprotka T, Delviks-Frankenberry KA, Cingoz O, Martinez A, Kung HJ, et al. (2011) Recombinant Origin of the Retrovirus XMRV. Science.
- 48. Sramkoski RM, Pretlow TG, 2nd , Giaconia JM, Pretlow TP, Schwartz S, et al. (1999) A new human prostate carcinoma cell line, 22Rv1. In Vitro Cell Dev Biol Anim 35: 403–409.
- 49. Pretlow TG, Wolman SR, Micale MA, Pelley RJ, Kursh ED, et al. (1993) Xenografts of primary human prostatic carcinoma. J Natl Cancer Inst 85: 394–398.
- 50. Nagabhushan M, Miller CM, Pretlow TP, Giaconia JM, Edgehouse NL, et al. (1996) CWR22: the first human prostate cancer xenograft with strongly androgen-dependent and relapsed strains both in vivo and in soft agar. Cancer Res 56: 3042–3046.
- 51. Knouf EC, Metzger MJ, Mitchell PS, Arroyo JD, Chevillet JR, et al. (2009) Multiple integrated copies and high-level production of the human retrovirus XMRV (xenotropic murine leukemia virus-related virus) from 22Rv1 prostate carcinoma cells. J Virol 83: 7353–7356.
- 52. Groom HC, Yap MW, Galao RP, Neil SJ, Bishop KN (2010) Susceptibility of xenotropic murine leukemia virus-related virus (XMRV) to retroviral restriction factors. Proc Natl Acad Sci U S A 107: 5166–5171.
- 53. Stieler K, Schulz C, Lavanya M, Aepfelbacher M, Stocking C, et al. (2010) Host range and cellular tropism of the human exogenous gammaretrovirus XMRV. Virology 399: 23–30.
- 54. Chaipan C, Dilley KA, Paprotka T, Delviks-Frankenberry KA, Venkatachari NJ, et al. (2011) Severe restriction of xenotropic murine leukemia virus-related virus replication and spread in cultured human peripheral blood mononuclear cells. J Virol 85: 4888–4897.
- 55. Ravichandran V, Major EO, Ibe C, Monaco MC, Girisetty MK, et al. (2011) Susceptibility of human primary neuronal cells to xenotropic murine leukemia virus-related (XMRV) virus infection. Virol J 8: 443.
- 56. Burtonboy G, Delferriere N, Mousset B, Heusterspreute M (1993) Isolation of a C-type retrovirus from an HIV infected cell line. Arch Virol 130: 289–300.
- 57. De Boer EC, Teppema JS, Steerenberg PA, De Jong WH (2000) Retrovirus type C in the mouse bladder carcinoma cell line MBT-2. J Urol 163: 1999–2001.
- 58. Deichmann M, Huder JB, Kleist C, Naher H, Schupbach J, et al. (2005) Detection of reverse transcriptase activity in human melanoma cell lines and identification of a murine leukemia virus contaminant. Arch Dermatol Res 296: 345–352.
- 59. Kotler M, Balabanova H, Ben-Moyal Z, Friedman A, Becker Y (1977) Properties of the oncornavirus particles isolated from P3HR-1 and Raji human lymphoblastoid cell lines. Isr J Med Sci 13: 740–746.
- 60. Raisch KP, Kushnaryov VM, Grossberg SE, Cashdollar LW (1998) Constitutive production of a murine retrovirus in the human B-lymphoblastoid cell line, DG-75. Virology 250: 135–139.
- 61. Takeuchi Y, McClure MO, Pizzato M (2008) Identification of gammaretroviruses constitutively released from cell lines used for human immunodeficiency virus research. J Virol 82: 12585–12588.
- 62. Yaniv A, Gotlieb-Stematsky T, Vonsover A, Perk K (1980) Evidence for type-C retrovirus production by Burkitt's lymphoma-derived cell line. Int J Cancer 25: 205–211.
- 63. Stocking C, Kozak CA (2008) Murine endogenous retroviruses. Cell Mol Life Sci 65: 3383–3398.
- 64. Baliji S, Liu Q, Kozak CA (2010) Common inbred strains of the laboratory mouse that are susceptible to infection by mouse xenotropic gammaretroviruses and the human-derived retrovirus XMRV. J Virol 84: 12841–12849.
- 65. Kozak CA, Hartley JW, Morse HC, 3rd (1984) Laboratory and wild-derived mice with multiple loci for production of xenotropic murine leukemia virus. J Virol 51: 77–80.
- 66. Levy JA (1999) Xenotropism: the elusive viral receptor finally uncovered. Proc Natl Acad Sci U S A 96: 802–804.
- 67. Oie HK, Russell EK, Dotson JH, Rhoads JM, Gazdar AF (1976) Host-range properties of murine xenotropic and ecotropic type-C viruses. J Natl Cancer Inst 56: 423–426.
- 68. Achong BG, Trumper PA, Giovanella BC (1976) C-type virus particles in human tumours transplanted into nude mice. Br J Cancer 34: 203–206.
- 69. Gautsch JW, Knowles AF, Jensen FC, Kaplan NO (1980) Highly efficient induction of type C retroviruses by a human tumor in athymic mice. Proc Natl Acad Sci U S A 77: 2247–2250.
- 70. Suzuki T, Yanagihara K, Yoshida K, Seido T, Kuga N (1977) Infectious murine type-C viruses released from human cancer cells transplated into nude mice. Gann 68: 99–106.
- 71. Todaro GJ, Arnstein P, Parks WP, Lennette EH, Huebner RJ (1973) A type-C virus in human rhabdomyosarcoma cells after inoculation into NIH Swiss mice treated with antithymocyte serum. Proc Natl Acad Sci U S A 70: 859–862.
- 72. Zhang YA, Maitra A, Hsieh JT, Rudin CM, Peacock C, et al. (2011) Frequent detection of infectious xenotropic murine leukemia virus (XMLV) in human cultures established from mouse xenografts. Cancer Biol Ther 12: 617–628.
- 73. Sfanos KS, Aloia AL, Hicks JL, Esopi DM, Steranka JP, et al. (2011) Identification of replication competent murine gammaretroviruses in commonly used prostate cancer cell lines. PLoS One 6: e20874.
- 74. Chiu YL, Greene WC (2008) The APOBEC3 cytidine deaminases: an innate defensive network opposing exogenous retroviruses and endogenous retroelements. Annu Rev Immunol 26: 317–353.
- 75. Stopak K, de Noronha C, Yonemoto W, Greene WC (2003) HIV-1 Vif blocks the antiviral activity of APOBEC3G by impairing both its translation and intracellular stability. Mol Cell 12: 591–601.
- 76. Wiegand HL, Doehle BP, Bogerd HP, Cullen BR (2004) A second human antiretroviral factor, APOBEC3F, is suppressed by the HIV-1 and HIV-2 Vif proteins. EMBO J 23: 2451–2458.
- 77. Rulli SJ Jr, Mirro J, Hill SA, Lloyd P, Gorelick RJ, et al. (2008) Interactions of murine APOBEC3 and human APOBEC3G with murine leukemia viruses. J Virol 82: 6566–6575.
- 78. Sheehy AM, Gaddis NC, Choi JD, Malim MH (2002) Isolation of a human gene that inhibits HIV-1 infection and is suppressed by the viral Vif protein. Nature 418: 646–650.
- 79. Dutko JA, Schafer A, Kenny AE, Cullen BR, Curcio MJ (2005) Inhibition of a yeast LTR retrotransposon by human APOBEC3 cytidine deaminases. Curr Biol 15: 661–666.
- 80. Esnault C, Heidmann O, Delebecque F, Dewannieux M, Ribet D, et al. (2005) APOBEC3G cytidine deaminase inhibits retrotransposition of endogenous retroviruses. Nature 433: 430–433.
- 81. Harris RS, Bishop KN, Sheehy AM, Craig HM, Petersen-Mahrt SK, et al. (2003) DNA deamination mediates innate immunity to retroviral infection. Cell 113: 803–809.
- 82. Mangeat B, Turelli P, Caron G, Friedli M, Perrin L, et al. (2003) Broad antiretroviral defence by human APOBEC3G through lethal editing of nascent reverse transcripts. Nature 424: 99–103.
- 83. Paprotka T, Venkatachari NJ, Chaipan C, Burdick R, Delviks-Frankenberry KA, et al. (2010) Inhibition of xenotropic murine leukemia virus-related virus by APOBEC3 proteins and antiviral drugs. J Virol 84: 5719–5729.
- 84. Stieler K, Fischer N (2010) Apobec 3G efficiently reduces infectivity of the human exogenous gammaretrovirus XMRV. PLoS One 5: e11738.
- 85. Bogerd HP, Zhang F, Bieniasz PD, Cullen BR (2011) Human APOBEC3 proteins can inhibit xenotropic murine leukemia virus-related virus infectivity. Virology 410: 234–239.
- 86. Onlamoon N, Das Gupta J, Sharma P, Rogers K, Suppiah S, et al. (2011) Infection, viral dissemination, and antibody responses of rhesus macaques exposed to the human gammaretrovirus XMRV. J Virol 85: 4547–4557.
- 87. Del Prete GQ, Kearney MF, Spindler J, Wiegand A, Chertova E, et al. (2012) Restricted Replication of Xenotropic Murine Leukemia Virus-Related Virus in Pigtailed Macaques. J Virol 86: 3152–3166.
- 88. Glushakova S, Baibakov B, Margolis LB, Zimmerberg J (1995) Infection of human tonsil histocultures: a model for HIV pathogenesis. Nat Med 1: 1320–1322.
- 89. Glushakova S, Baibakov B, Zimmerberg J, Margolis LB (1997) Experimental HIV infection of human lymphoid tissue: correlation of CD4+ T cell depletion and virus syncytium-inducing/non-syncytium-inducingphenotype in histocultures inoculated with laboratory strains and patient isolates of HIV type 1. AIDS Res Hum Retroviruses 13: 461–471.
- 90. Grivel JC, Santoro F, Chen S, Faga G, Malnati MS, et al. (2003) Pathogenic effects of human herpesvirus 6 in human lymphoid tissue ex vivo. J Virol 77: 8280–8289.
- 91. Rose PP, Korber BT (2000) Detecting hypermutations in viral sequences with an emphasis on G→A hypermutation. Bioinformatics 16: 400–401.
- 92. Singh IR, Gorzynski JE, Drobysheva D, Bassit L, Schinazi RF (2010) Raltegravir is a potent inhibitor of XMRV, a virus implicated in prostate cancer and chronic fatigue syndrome. PLoS One 5: e9948.
- 93. Sakuma R, Sakuma T, Ohmine S, Silverman RH, Ikeda Y (2010) Xenotropic murine leukemia virus-related virus is susceptible to AZT. Virology 397: 1–6.
- 94. Hazuda DJ, Felock P, Witmer M, Wolfe A, Stillmock K, et al. (2000) Inhibitors of strand transfer that prevent integration and inhibit HIV-1 replication in cells. Science 287: 646–650.
- 95. Koning FA, Newman EN, Kim EY, Kunstman KJ, Wolinsky SM, et al. (2009) Defining APOBEC3 expression patterns in human tissues and hematopoietic cell subsets. J Virol 83: 9474–9485.
- 96. Grivel JC, Biancotto A, Ito Y, Lima RG, Margolis LB (2003) Bystander CD4+ T lymphocytes survive in HIV-infected human lymphoid tissue. AIDS Res Hum Retroviruses 19: 211–216.
- 97. Grivel JC, Elliott J, Lisco A, Biancotto A, Condack C, et al. (2007) HIV-1 pathogenesis differs in rectosigmoid and tonsillar tissues infected ex vivo with CCR5- and CXCR4-tropic HIV-1. AIDS 21: 1263–1272.
- 98. Ito Y, Grivel JC, Chen S, Kiselyeva Y, Reichelderfer P, et al. (2004) CXCR4-tropic HIV-1 suppresses replication of CCR5-tropic HIV-1 in human lymphoid tissue by selective induction of CC-chemokines. J Infect Dis 189: 506–514.
- 99. Lombardi VC, Hagen KS, Hunter KW, Diamond JW, Smith-Gagen J, et al. (2011) Xenotropic Murine Leukemia Virus-related Virus-associated Chronic Fatigue Syndrome Reveals a Distinct Inflammatory Signature. In Vivo 25: 307–314.
- 100. Brenu EW, van Driel ML, Staines DR, Ashton KJ, Ramos SB, et al. (2011) Immunological abnormalities as potential biomarkers in Chronic Fatigue Syndrome/Myalgic Encephalomyelitis. J Transl Med 9: 81.
- 101. Battini JL, Rasko JE, Miller AD (1999) A human cell-surface receptor for xenotropic and polytropic murine leukemia viruses: possible role in G protein-coupled signal transduction. Proc Natl Acad Sci U S A 96: 1385–1390.
- 102. Rodriguez JJ, Goff SP (2010) Xenotropic murine leukemia virus-related virus establishes an efficient spreading infection and exhibits enhanced transcriptional activity in prostate carcinoma cells. J Virol 84: 2556–2562.
- 103. Zhao C, Papadopoulou B, Tremblay MJ (2004) Leishmania infantum promotes replication of HIV type 1 in human lymphoid tissue cultured ex vivo by inducing secretion of the proinflammatory cytokines TNF-alpha and IL-1 alpha. J Immunol 172: 3086–3093.