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Research Article

Successful Isolation of Infectious and High Titer Human Monocyte-Derived HIV-1 from Two Subjects with Discontinued Therapy

  • Tong Wang equal contributor,

    equal contributor Contributed equally to this work with: Tong Wang, Younong Xu

    Affiliations: Department of Laboratory Medicine, University of Washington, Seattle, Washington, United States of America, Key Laboratory of Functional Protein Research of Guangdong Higher Education Institutes, Guangzhou, Guangdong, China, Institute of Life and Health Engineering, College of Life Science and Technology, Jinan University, Guangzhou, Guangdong, China

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  • Younong Xu equal contributor,

    equal contributor Contributed equally to this work with: Tong Wang, Younong Xu

    Affiliation: Department of Laboratory Medicine, University of Washington, Seattle, Washington, United States of America

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  • Haiying Zhu,

    Affiliation: Department of Laboratory Medicine, University of Washington, Seattle, Washington, United States of America

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  • Thomas Andrus,

    Affiliation: Department of Laboratory Medicine, University of Washington, Seattle, Washington, United States of America

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  • Sergei B. Ivanov,

    Affiliation: Department of Laboratory Medicine, University of Washington, Seattle, Washington, United States of America

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  • Charlotte Pan,

    Affiliation: Department of Laboratory Medicine, University of Washington, Seattle, Washington, United States of America

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  • Jazel Dolores,

    Affiliation: Department of Laboratory Medicine, University of Washington, Seattle, Washington, United States of America

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  • Gregory C. Dann,

    Affiliation: Department of Laboratory Medicine, University of Washington, Seattle, Washington, United States of America

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  • Michael Zhou,

    Affiliation: Department of Laboratory Medicine, University of Washington, Seattle, Washington, United States of America

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  • Dominic Forte,

    Affiliation: Department of Laboratory Medicine, University of Washington, Seattle, Washington, United States of America

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  • Zihuan Yang,

    Affiliation: Department of Laboratory Medicine, University of Washington, Seattle, Washington, United States of America

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  • Sarah Holte,

    Affiliations: Department of Biostatistics, University of Washington, Seattle, Washington, United States of America, Division of Public Health Sciences, Fred Hutchinson Cancer Research Center, Seattle, Washington, United States of America

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  • Lawrence Corey,

    Affiliations: Department of Laboratory Medicine, University of Washington, Seattle, Washington, United States of America, Division of Vaccine and Infectious Disease Division, Fred Hutchinson Cancer Research Center, Seattle, Washington, United States of America

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  • Tuofu Zhu mail

    tzhu@u.washington.edu

    Affiliations: Department of Laboratory Medicine, University of Washington, Seattle, Washington, United States of America, Division of Vaccine and Infectious Disease Division, Fred Hutchinson Cancer Research Center, Seattle, Washington, United States of America

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  • Published: May 31, 2013
  • DOI: 10.1371/journal.pone.0065071

Abstract

Background

HIV-1 DNA in blood monocytes is considered a viral source of various HIV-1 infected tissue macrophages, which is also known as “Trojan horse” hypothesis. However, whether these DNA can produce virions has been an open question for years, due to the inability of isolating high titer and infectious HIV-1 directly from monocytes.

Results

In this study, we demonstrated successful isolation of two strains of M-HIV-1 (1690 M and 1175 M) from two out of four study subjects, together with their in vivo controls, HIV-1 isolated from CD4+ T-cells (T-HIV-1), 1690 T and 1175 T. All M- and T- HIV-1 isolates were detected CCR5-tropic. Both M- HIV-1 exhibited higher levels of replication in monocyte-derived macrophages (MDM) than the two T- HIV-1. Consistent with our previous reports on the subject 1175 with late infection, compartmentalized env C2-V3-C3 sequences were identified between 1175 M and 1175 T. In contrast, 1690 M and 1690 T, which were isolated from subject 1690 with relatively earlier infection, showed homogenous env C2-V3-C3 sequences. However, multiple reverse transcriptase (RT) inhibitor resistance-associated variations were detected in the Gag-Pol region of 1690 M, but not of 1690 T. By further measuring HIV DNA intracellular copy numbers post-MDM infection, 1690 M was found to have significantly higher DNA synthesis efficiency than 1690 T in macrophages, indicating a higher RT activity, which was confirmed by AZT inhibitory assays.

Conclusions

These results suggested that the M- and T- HIV-1 are compartmentalized in the two study subjects, respectively. Therefore, we demonstrated that under in vitro conditions, HIV-1 infected human monocytes can productively release live viruses while differentiating into macrophages.

Introduction

Peripheral blood monocytes can enter a variety of tissues across capillary endothelial walls, undergoing differentiation to become tissue-specific resident macrophages, such as microglia and perivascular macrophages in the brain, alveolar macrophages in the lung and Kupffer cells in the liver [1], [2]. Based on these migration and differentiation phenotypes, early investigations implicated HIV-1 infected monocytes, carrying provirus, might be able to differentiate into tissue macrophages and develop HIV-1 productive infection in situ [3][14]. As such, HIV-1 in blood monocytes is considered as a source of progeny viruses in various tissues.

We and others have shown that HIV-1 DNA in patient monocytes are genetically distinct from those derived from CD4+ T cells [15][20]. These DNA may have the potential to be activated and release progeny virions. Evidence include studies from us and others [15][18], [20] demonstrating that monocyte/macrophages (M/M) are one of the major sources of HIV-1 in vivo, particularly in patients receiving highly active antiretroviral therapy (HAART). This deduction is also supported by the fact that the HIV-1 DNA in circulating monocytes has been identified as one of the mechanisms of HIV-1-associated neurocognitive disturbances (HAND) progression [21] and other M/M associated HIV diseases, such as atherosclerosis (reviewed in [22]). Etiologically, although whether these viral DNA in monocytes could produce virions or not is unknown, consistent replenishment of replicable HIV-1 in the central nervous system (CNS) was proposed to be associated with CNS viral persistence and the neurotoxic host inflammatory responses [23][27]. On the other hand, reverse trans-endothelial migration of HIV-1 infected M/M was also reported by employing an in vitro blood brain barrier (BBB) model, suggesting the possibility that monocytic trafficking from the brain to the periphery may be partially responsible for the rebound of blood viremia [27].

These processes are also known as the “Trojan horse” hypothesis (reviewed in [28][31]). Several laboratory-adapted strains have been employed to substantiate this hypothesis in investigative systems including trans-endothelial and co-cultivation models [27], [32][35]. However, the in vivo relevance of applying these models to neuroAIDS studies could be improved by overcoming a major technological hindrance that has existed for more than two decades: the inability to isolate primary HIV-1 from monocytes that may grow substantially in vitro.

Equally important is that HIV-1 DNA in M/M can persist for long periods without integrating, while producing viral mRNAs and proteins as reported recently [36], [37]. The transcriptional products in this process could be detected by PCR, leading to a conclusion of productive infection, however with no progeny virion release examined. Lambotte et al [38] and Sonza et al [39] have independently reported the isolation of infection-competent HIV-1 from the monocytes of patients while receiving effective HAART. These HIV-1 isolates were at PCR-detectable levels and no infectivity data were reported [38], [39]. While these studies are significant, the transcription of latent HIV-1 DNA that results in viral mRNA release should be considered [36], [37]. Addressing this question warrants direct evidence that monocytes can release virions during the differentiation process to macrophages. This is also a prerequisite of the “Trojan horse” hypothesis if the monocyte-derived HIV-1 DNA is a substantial source of brain HIV-1.

It is known that activated CD4+ T cells are capable of sustaining rapid and exponential HIV-1 production [40][42], and latently infected CD4+ T cells, including resting and central memory T cells, are viral reservoirs in the peripheral blood [43][51]. However, later studies indicated that in patients with suppressive HAART, non-CD4+ T lymphocytes, including M/M, are the major sources of plasma HIV-1 [15], [20], [50], [52] (reviewed in [19], [53], [54]). These findings emphasize the possibility that HIV-1 DNA harbored by monocytes may be a source of live viruses responsible for viral rebound post-discontinued therapy, which has not been substantiated to date.

Therefore, we focused on our well-studied subjects [15], [17], [18], [20] in this study and described the successful isolation of monocyte-derived primary HIV-1 (M- HIV-1) and their in vivo controls, CD4+ T cell-derived primary HIV-1 (T- HIV-1), from two out of four study subjects. These findings are direct evidence of monocytic release of HIV-1 live viruses, which is favorable to the “Trojan horse” hypothesis in HIV-1 tissue transmission.

Results

Isolation of HIV-1 from Purified Patient Monocytes and CD4+ T cells

Peripheral blood mononuclear cell (PBMC) samples of Subjects 1175, 1690, 1696 and 1155 from the Seattle Primary Infection Cohort (SeaPIC) [55], [56], who received discontinued therapy, were used for viral isolation. The scientific and ethics review committees of the University of Washington approved this study, and written informed consents were obtained from the study participants. We complied with the human experimentation guidelines of the US Department of Health and Human Services when obtaining clinical samples.

As M-HIV-1 isolation was only successful in Subject 1175 and 1690, their treatment information and sampling time points were summarized in Figure 1. In general, the viral loads of both subjects were successfully suppressed to less than 50 copies/ml by HAART, followed by viral load rebound with discontinued therapy. As mentioned in the introduction section, these viruses were rebounded primarily from non-CD4+ T cells and most likely derived from monocytes [15][18], [20]; this may increase the probability for viral isolation from monocytes. Thus, we acquired PBMC samples for viral isolation at the time points with the longest duration of discontinued therapy for both subjects.

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Figure 1. Viral isolation from Subject 1175 and 1690.

Clinical information of study Subject 1175 (A) and 1690 (B). For each subject, the first visit with confirmative diagnosis of seroconversion, along with the corresponding HIV-1 RNA viral load, is plotted at Month 0. Subsequently, longitudinal visits, viral loads, treatment and sampling time points are shown. (C) The monocyte purification strategy. Non-monocytes were magnetically labeled and removed from PBMCs of 2 healthy donors. The eluent monocytes were positively sorted and subjected to a four-hour attachment purification followed by two intensive washes with PBS. Percentage of T cell contamination before and after attachment purification was shown in the shaded quadrants of each flow cytometry graph. Monocyte- and CD4+ T cell-derived HIV-1 were obtained from subject 1175 (D) and 1690 (E) by being co-cultivated with CD8+ T cell-depleted donor PBMC. Longitudinal HIV-1 p24 concentrations in supernatants were shown for each co-cultivation. The high limit cut-off of HIV-1 p24 concentration is 20 ng/ml and lower limit for detection (LLD) is 0.01 ng/ml. The time points for viral expansion and stock preparation were indicated with dash lines with arrowheads. TCID50 titers of each viral expansion of 1175 T and 1175 M (D), as well as 1690 T and 1690 M (E), are shown in each corresponding box.

doi:10.1371/journal.pone.0065071.g001

In detail, from 334 to 1001 d post-seroconversion (PSC), subject 1175 was treated with Indinavir, Lamivudine and Zidovudine, followed by a period with no therapy until 3407 d PSC. The subject initiated a second therapy regimen of Efavirenz, Epzicom and Kivexa at 3596 d PSC, the same time point that PBMC samples were acquired for virus isolation (immediately before therapy) (Figure 1A). Subject 1690 was treated with Kaletra and Combivir from 29 d to 166 d PSC, stopped therapy for 188 d, and initiated the same therapy regimen from 336 d PSC (Figure 1B). PBMC samples for 1690 were acquired 295 d PSC (Figure 1B). Plasma viral loads of the two subjects at their respective sampling time points for viral isolation were 1.3×105 copies/ml for 1175 (Figure 1A) and 1.9×105 copies/ml for 1690 (Figure 1B).

We have optimized CD14+ monocyte purification by using a two-step, magnetic bead-based cell sorting strategy as previously described [15], [17], [20]. In addition, we included an attachment purification procedure to further remove non-monocyte cell populations. The overall monocyte isolation strategy is shown in Figure 1C.

We validated this strategy with 2 healthy donors by analyzing T cell contamination using flow cytometry (FACS). The feasibility of this validation capitalizes on an interesting feature of monocyte-derived macrophages (MDM) in vitro culture. Monocytes will attach to the bottom of the culture surface rapidly (>95% adherence rate at 4 h post seeding), however, over 80% of these attached cells will be released back into culture media 24–48 h post-seeding. Following differentiation, viable MDM will again adhere to the culture surface and remain attached for more than 30 d. This adherence quality allowed us to collect cells after attachment purification for FACS assay at 24 h post-seeding without disturbing cell surface markers. CD3+CD14 T cells were grouped in the upper left quadrant of each FACS graph (Figure 1C). For Donor 1, prior to the attachment purification, there was less than 0.1% T cell contamination was detected, however non-detectable T cell contamination was observed after attachment purification (Figure 1C). No T cell contamination was detected either before or after attachment purification in Donor 2 (Figure 1C). We further employed reverse transcription PCR (RT-PCR) to determine T cell receptor (TCR) mRNA levels in the purified monocyte populations, as described [18], and found no detectable TCR mRNA in the purified monocytes of either donors. With this optimized method, we can acquire purified monocytes with no detectable T cell contamination.

We then used this methodology to purify monocytes from all subjects for viral isolation. No detectable TCR mRNA in the purified monocytes of each subject was observed. Out of the four subjects, M-HIV-1 were successfully isolated from two of them (1175 and 1690). HIV-1 primary isolates were defined as either M (monocyte) or T (CD4+ T cell-derived) following the subject ID, that is: 1175 M and 1175 T, or 1690 M and 1690 T represent M- and T- derived HIV-1 isolated from subjects 1175 and 1690, respectively. M- and T- derived HIV-1 were successfully isolated based on p24 ELISA positivity and 50% tissue culture infectious dose (TCID50) viral titration (Figure 1D and 1E). By monitoring HIV-1 p24 production in the supernatants, the co-culture for isolating 1175 T first showed p24 ELISA positive on Day 5, while 1175 M was positive on Day 18 (Figure 1D). Comparably, p24 positivity was observed on Day 12 for 1690 T co-culture and Day 13 for 1690 M (Figure 1E). To maximally avoid mutation interference, we collected primary isolates at the first time point of each experiment when p24 production was positively detected. Titers of each viral expansion used for subsequent virological and biological evaluations are indicated by TCID50/ml: 1175 T (6.3×105), 1175 M (7.4×103), 1690 T (1.4×104) and 1690 M (3.0×104) TCID50/ml (Figure 1D&E).

Co-receptor Use Prediction and Biological Confirmation

By analyzing the sequences of env V3 regions of each HIV-1 isolate, theoretical phenotypes including the syncytium-inducing (SI) effects and co-receptor usage of each isolate were calculated (Table 1.). According to the 11/25 rule [57], 1690 M and 1690 T are non-syncytium-inducing (NSI) viruses; however, 1175 M and 1175 T are SI viruses (Table 1.). In terms of Geno2pheno prediction [58], 1690 M and 1690 T were R5-tropic HIV-1, while 1175 M and 1175 T were predicted as CXCR4 (X4)-tropic viruses (Table 1.). PSSM prediction [59] indicated that 1175 M and 1175 T were CCR5 (R5)-tropic HIV-1, although consistent R5-tropic predictions with Geno2pheno were made for 1690 M and 1690 T (Table 1.). We next biologically evaluated the co-receptor usage of HIV-1 isolates by performing in vitro infection experiments with the U87 and U373-MAGI cell lines (Table 1.). Multiple negative and positive controls were used to confirm the validity of the two indicator cell lines as described in the Material and Methods. All of the four isolates could only infect and replicate in U87-CCR5 and U373 MAGI.CCR5 cells, demonstrating R5-tropism (Table 1.).

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Table 1. HIV-1 Env V3 amino acid sequences with computational and biological prediction of co-receptor usage.

doi:10.1371/journal.pone.0065071.t001

Replication Kinetics in MDM Infection

To validate whether the M- and T- HIV-1 were isolated from different compartments, we compared the phenotypic difference, as the first step, between these isolates by infecting MDM that were prepared from 4 individual healthy donors, respectively; as a positive control, parallel experiments were performed with HIV-1 BaL (Figure 2).

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Figure 2. Observation of replication kinetics in MDM.

HIV-1 p24 production kinetics in MDM was shown for1690 M (A) and1690 T and 1175 M and 1175 T (B). Seven-day old MDM infection at MOI = 0.01 for 4 h before continuously cultured in fresh media. Supernatant HIV-1 p24 concentrations were determined and shown longitudinally (ng/mL, mean ± SEM, donor n = 4). (C) Supernatant viral RNA copy numbers of MDM infections. Supernatant samples were acquired on Day 22 post-infection and data were shown as copies/mL (donor n = 3). (D) Viral replication in PHA-PBMC. Donor PBMCs were stimulated by PHA for 48 h before BaL, 1690 M, 1690 T, 1175 M and 1175 T infections at MOI = 0.01. HIV-1 p24 concentrations in culture supernatants on Day 7 post-infection were shown (ng/mL, mean ± SEM). *P<0.05, donor n = 4 compared with the BaL-infected group. E, Intracellular staining of HIV-1 p24. MDM were infected for 14 d before cyto-immunochemistry staining with CD14 (red), DAPI (blue) and HIV-1 p24 (green). Scale bar = 20 µm.

doi:10.1371/journal.pone.0065071.g002

Using a linear model and generalized estimating equations (GEE) with exchangeable correlation structure for repeated measures from the same donor [60], the 1690 M infected group showed significantly higher HIV-1 p24 production than the 1690 T group, longitudinally (P<0.01, donor n = 4, Figure 2A). The 1175 M and 1175 T infected groups showed p24 production at levels close to the ELISA lower limit of detection (LLD, 0.01 ng/ml) for most of the time points; and the 1175 M infected MDM showed a general pattern of higher p24 production than the 1175 T infected group (Figure 2B), especially on Day 18 post-infection (P<0.05, donor n = 4). The HIV-1 infected MDM were observed to maintain healthy morphologies until Day 22 post-infection, and gradually show cytotoxic morphologies thereafter, such as shrinkage and decrease in cell numbers. As such, to validate the replication difference between M- and T- HIV-1, we used quantitative PCR to examine supernatant viral RNA copy numbers on Day 22 post-infection in the 1690 M, 1690 T, 1175 M and 1175 T infected MDM (Figure 2C). The comparison was performed with linear regression and GEE with exchangeable correlation structure for repeated measures from the same donor, within virus from the same patient. The average viral RNA copy number of the M-HIV-1 infected groups was 1.1×104 copies/ml, which is significantly higher than the T-HIV-1 infected groups (5.8×102 copies/ml) (P<0.01, donor n = 3, Figure 2C).

As 1175 M, 1175 T and 1690 T showed only moderate RNA or p24 production in MDM, we need test whether these are defective viruses or not. Thus, infection experiments by using PHA-stimulated PBMCs were performed, and peripheral blood from four different healthy donors were used for this validation (Figure 2D). On Day 7 post-infection, supernatant p24 production was seen in the 1690 T (236±19 ng/mL), 1690 M (201±47 ng/mL), 1175 T (355±17 ng/mL) and 1175 M (190±18 ng/mL) infected groups (Figure 2D). These results demonstrate the four primary isolates are replication-competent viruses.

To visualize the viral replication in MDM, we adopted cyto-immunochemistry to assay the HIV-1 p24 production (Figure 2E). As a negative control, uninfected monocytes from healthy donors were allowed to differentiate for 21 d before observation. High power fields (HPF) of observations indicated multinucleated giant cells expressing both CD14 and HIV-1 p24 were observed in the BaL-, 1690 M- and 1690 T- infected MDM, respectively (Figure 2E). These results verified that supernatant p24 and viral production is due to MDM productive infection.

Genetic Characterization of M- and T- derived HIV-1 env C2-V3-C3 Regions

We next performed HIV-1 sequence analysis on the env C2-V3-C3 regions of all of the four primary isolates (1175 M, 1175 T, 1690 M and 1690 T) to detect compartmentaliztion (Figure 3). In addition, to identify the viruses that are replication-competent in macrophages, the MDM selection of the primary M- and T- isolates were used to differentiate the strains that could productively infect MDM (Figure 3). Sequence comparisons with our published proviral sequences [15], [17], [20] were performed to investigate the cell type-specific origin of the isolates (Figure 3). The MDM selection experiments were independently performed for three times using blood M/M from three different healthy donors, respectively (Figure 3).

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Figure 3. Phylogenetic analysis of HIV-1 env C2-V3-C3 sequences of monocyte- and CD4+ T cell-derived HIV-1.

The neighbor-joining trees of 1175 M and 1175 T (A) as well as 1690 M and 1690 T (B) were shown, respectively. The env C2-V3-C3 sequences of provirues as well as primary isolate before and after MDM selection were acquired from limiting dilution PCR. MDM selection experiments were using seven-day old MDM prepared from 3 healthy donors, respectively, at MOI = 0.01. On Day 22 post-infection, supernatants of infected MDM were subjected to sequence analysis. The viral nucleotide sequences were used to construct neighbor-joining trees based on nucleotide pairwise distances. Reference sequences (not labeled) are HIV-1 subtype B sequences from GenBank database (http://www.ncbi.nlm.nih.gov/).

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In order to eliminate re-sampling and PCR-caused errors, we employed our well-established limiting-dilution PCR strategies [15], [17], [20]; each of the end-point diluted PCR products was directly sequenced. We observed identical V3 sequences within limiting-diluted PCR reactions of each isolate. Consistent with our previous reports [15], [17], [20], heterogeneous sequences of HIV-1 env C2-V3-C3 regions of the proviruses in the monocytes and CD4+ T cells of both 1175 and 1690 were observed (Figure 3A and 3B). Sequence diversities of proviruses from monocytes were 2.08% and 1.79% in 1175 and 1690, respectively. The diversities of proviruses from CD4+ T cells were 3.47% and 2.22% in 1175 and 1690, respectively. There were also notable sequence variations of HIV-1 env C2-V3-C3 regions from 1175 T (3.48% diversity) and after MDM selection (1.73% in Donor 1 and 1.44% in Donor 2, negative in Donor 3 MDM cultures). On the contrary, before MDM selection, 1175 M showed relatively homogenous sequences (0.8% diversity); however, 1175 M produced more homogenous sequences after MDM selection (0.12% diversity in Donor 1, 0.13% diversity in Donor 2 and 0.06% diversity in Donor 3 MDM cultures) (Figure 3A). Regarding 1175 isolates, we observed only strains with similar sequences to 1175 M could survive the MDM selection. These env C2-V3-C3 sequence results indicate 1175 M exists as minor strains of HIV-1 in peripheral blood of subject 1175 and are genetically distinct from 1175 T. The 1175 M strains are capable of replicating in MDM with higher MDM fitness than 1175 T strains from the same subject.

In contrast, homogenous env C2-V3-C3 sequences were detected before MDM selection in 1690 M (0.16% diversity) and 1690 T (0.14% diversity), as well as after MDM selection in 1690 M (0.00%,0.15% and 0.35% diversity for Donor1, Donor 2 and Donor 3, respectively) and 1690 T (0.20%, 0.17% and 0.00% diversity for Donor1, Donor 2 and Donor 3, respectively) (Figure 3B).

Genotypic Differences in the Infectivity-related gag-pol Region of MDM Selected 1690 M and 1690 T

As similar env C2-V3-C3 sequences between1690 M and 1690 T were detected, we next examined the gag-pol variations to further define the genotypic difference between the two isolates. The consensus sequences of MDM-selected 1690 M and 1690 T were analyzed by directly sequencing PCR products in the supernatants of infected MDM prepared from three healthy donors (Figure 4). The variations after MDM selection between 1690 M and 1690 T shown are consistently detected among all three donors (Figure 4). After MDM selection, a total of seven variations comparing 1690 T with 1690 M were detected in the reverse transcriptase (RT) coding region: L178I, V179I, G190A, T200A, I293V and T297E (Figure 4A&B), as well as I142T (Figure 4C). Five variations were detected in the Gag-Pol trans-frame region: R28S, R35G, G36R, R41P and T44A (Figure 4D). Other observed variations include I64V in the protease region (Figure 4E), R18Q in the Gag-spacer peptide p2 encoding region (Figure 4F), as well as E97A and A110P in the p6 encoding region (Figure 4G).

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Figure 4. Deduced amino acid sequence alignment of HIV-1 Gag-Pol regions of MDM-selected 1690 M and 1690 T.

Amino acid sequence differences between MDM selected 1690 M and 1690 T were shown in the regions of reverse transcriptase (A-C), Gag-Pol trans-frame (D), protease (E), Gag p2 (F) and Gag p6 (G). MDM from 3 different donors (Donor 1, 2 and 3) were infected with 1690 M and 1690 T, respectively. Supernatants were harvested on Day 22 post-infection and subjected to RT-PCR and sequence analysis on Gag-Pol regions of HIV-1. (2/2) represents the same individual sequences were detected from two RT-PCR. Differential residuals were indicated by both “*” and position numbers aligned with HXB2 sequences.

doi:10.1371/journal.pone.0065071.g004

Intracellular HIV-1 DNA Production in MDM and RT Activity Difference Comparing 1690 M with 1690 T

Our genetic analyses of 1690 M and 1690 T allowed us to hypothesize that the phenotype difference between the two viruses in MDM is partially due to the RT activity difference. Thus, we further tested the intracellular HIV cDNA production in MDM longitudinally (Figure 5). To calculate intracellular viral cDNA copy numbers in MDM, our published PCR strategy by simultaneously analyzing HIV-1 p24 and p17 cDNA was employed [20], [61]. These experiments were independently repeated for three times, each using MDM prepared from one of the three healthy donors.

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Figure 5. Intracellular viral DNA persistence in MDM acute infection and longitudinal reverse transcriptase activity assay.

(A) HIV-1 DNA synthesis kinetics in MDM. Seven-day old MDM from 3 healthy donors were infected by 1690 M and 1690 T, respectively, at MOI = 0.01. Cells were harvested at 2 h, 4 h, 8 h, 12 h, 24 h, 48 h, 72 h and 168 h post-infection. Intracellular HIV-1 DNA copy numbers were determined. *P<0.05, donor n = 3. (B) Viral resistance to azidothymidine. Seven-day old MDM were infected by 1690 M and 1690 T, respectively, at MOI = 0.01. On Day 6 post-infection, supernatants were removed and MDM were exposed to AZT at serially diluted concentrations as indicated. The inhibition rates calculated by relative p24 production were shown for the time points of Day 8, 12 and 16 post-infection, respectively. Data were shown as mean ± SEM, donor n = 3.

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Although donor difference was observed, MDM infected with 1690 M showed either significantly higher intracellular DNA copy numbers or no statistical difference from 1690 T-infected MDM, longitudinally (Figure 5A). When evaluating early infection time points, 1690 M showed significantly higher DNA production in MDM than 1690 T at 4 h (P<0.01, n = 3), however the absolute amount of intracellular viral DNA decreased from 4–12 h and no significant viral DNA level difference was detected at 12 h post-infection (Figure 5A).

Such significant fluctuations in viral DNA production may be a result of RT activity differences, both in acute and chronic phases post-infection in MDM. In this regard, we performed a longitudinal infection of MDM using 1690 M and 1690 T in the presence of the RT inhibitor, azidothymidine (AZT) (Figure 5B). These experiments were independently repeated three times, each using MDM prepared from one of the three healthy donors. On Day 8 post-infection, the EC50 of AZT in blocking RT activity in the 1690 M-infected MDM group was 6.70 nM, significantly higher than the 1690 T group (0.28 nM, P<0.01, donor n = 3) (Figure 5B). Similar RT activity differences were detected in the latter time points: 0.70 nM in the 1690 M group and 0.27 nM in the 1690 T group on Day 12 (P<0.01, n = 3), as well as 2.7 nM versus 0.32 nM on Day 16 (P<0.01, n = 3) (Figure 5B). These results indicate that the RT activity of 1690 M is significantly higher than that of 1690 T.

Discussion

Currently used HAART regimens fail to effectively inhibit HIV-1 DNA persistence in monocytes, while suppressing HIV-1 in CD4+ T cells well [15][17], [20], [62][65].Our findings in this study pointed toward that these HIV-1 DNA in monocytes are not only transcription-competent, but also capable of producing live viruses along with the monocytic differentiation. This is evidenced by the isolation of M- HIV-1 with both nanogram p24 level and high infectious titers, although only successful in two study subjects. Per these results, we could conclude that the monocytic HIV-1 DNA is an active source of virions in HIV-1 brain transmission. To explain the origin of these viral DNA, Carter et al found that the multipotent hematopoietic progenitor cells (HPCs) can be productively infected by HIV-1 [66]. In comparison, recent findings suggested another two types of “Trojan horses”, showing that infected macrophages can migrate inside-out and outside-in the brain [27], and macrophage-derived exosomes and microvesicles are also active vehicles for HIV-1 to mediate productive infection [67]. Taking these together, brain infection of HIV-1 involves in sophisticated mechanisms, but the possibility of viral replenishment via monocytes is confirmed by our findings.

According to the data of subject 1175 we previously reported [17], HIV-1 DNA in monocytes and CD4+ T cells had homogenous sequences in the env C2-V5 regions during acute infection stages, however significant compartmentalization and variation were found in late stages [17]. This is biologically comparable with our findings here: 1) patient cells utilized for 1175 viral isolation were acquired from late stages of infection, and the proviruses in monocytes and CD4+ T cells were known to exhibited compartmentalization [17]; 2) although diversified proviruses were observed in monocytes, homogenous sequences were detected in 1175 M, in contrast to the multiple variants that were isolated in 1175 T. Favorable to our conclusions, there were reports indicating a number of R5 strains found in HIV-1 infected patients cannot enter macrophages at early stages; however, macrophage entry capacity was observed to be increasing longitudinally throughout disease progression [68], [69]. In addition, macrophages are known to express both CCR5 and CXCR4; early investigations by using HIV-1 isolates showed HIV-1 is being adapted to use CXCR4 in addition to CCR5 expressed by both macrophages and CD4+ T cells along with infection progression [70], [71]. Adding to this knowledge, our results demonstrated strong monocytic selection on HIV-1 in vivo. This is in agreement with the facts that the failure of productive infection of HIV-1 in monocytes is due to post-entry events [72], [73].

Samples for viral isolation were acquired from relatively early infection for Subject 1690; we observed homogenous env C2-V3-C3 sequences between 1690 M and 1690 T as anticipated. Therefore, the phenotypic difference between the two isolates could be partially explained by replication-associated variation in viral sequences. We demonstrated that 1690 M has more resistance variation sites than those from CD4+ T cells. These sites include the well documented non-nucleoside RT inhibitor (NNRTI) resistance-associated mutation, G190A [74][76], when comparing 1690 T with 1690 M, as well as four others that are known to confer lesser degrees of NNRTI resistance, including V179I [77], I293V [78] and T200I [77]. In addition, the I64V mutation in the protease region was also reported to be relevant to protease inhibitor resistance [79]. Indeed, it is known that acquiring these mutations is to be beneficial for HIV-1 by increasing fitness in host cells, representing a monocyte selection mechanism of concentrating viruses that have higher RT activity [39].

This was supported by the results of HIV-1 DNA copy number calculation post-entry. We found the 1690 M-infected MDM showed significantly higher viral DNA production than those in the 1690 T group for the first 4 h post-infection. It has been reported that the minimum duration of an HIV-1 replication cycle in vivo is about 1.2 d and the average duplication time is 2.6 d [42]. During this process, reverse transcription requires nearly 4 h in both CD4+ T cells and mononuclear phagocytes [42], [80]. However, subsequent events, including integration and progeny viral assembly, are slower in the latter [80]. As DNA production in the 4 h time window is completely dependent on the efficiency of reverse transcription, RT activity difference between 1690 M and 1690 T became a focus of mechanistic probing in this study. Notably, by employing the RT inhibitor AZT, we validated that 1690 M has higher RT activity than 1690 T.

Timely and sufficient reverse transcription is a crucial prerequisite for the survival of HIV-1 in monocytes [81]. It has been demonstrated that HIV-1 post-entry block in monocytes occurs prior to or during the reverse transcription phase [9], [72], [81]. Slower DNA synthesis results in increased DNA degradation, while insufficient reverse transcription leads to integration block and increased levels of unintegrated DNA. Compared with macrophages, there are abundant factors in monocytes that may confer the inhibition of reverse transcription. They include lower levels of dTTP [9], higher levels of APOBEC3A and APOBEC3G [82], [83] as well as the recently identified HIV-1 reverse transcription restriction factor, SAM- and HD-domain-containing protein (SAMHD1) [84], [85]. Therefore, to meet the requirement of the rate and quality of viral DNA production for survival in monocytes, higher RT activity is demanded. This is in agreement with our previous report indicating that after prolonged HAART, HIV-1 variants related or identical to those found only in CD14+ monocytes were also seen in plasma from treated subjects, suggesting that HIV-1 in circulating monocytes represent replicating virus that were able to survive with effective HAART [20].

In conclusion, the above-mentioned genotype and phenotype results confirmed that the M- and T- HIV-1 were isolated from different cellular compartments in the two subjects, respectively. Therefore, we demonstrated that infectious HIV-1 can be recovered from the monocytes of infected patients. These findings are the first biological evidence of monocyte-derived HIV-1, leading to a better understanding of cell-specific viral persistence and the “Trojan horse” hypothesis in HIV-1 CNS transmission. The M-HIV-1 may be applied to neuroAIDS and other HIV-1 disease modeling systems, as well as further benefit the biological and pharmaceutical evaluation of monocyte/macrophage-related HIV-1 pathogenesis.

Materials and Methods

Isolation of Infectious HIV-1 from Purified Monocytes

CD14+ monocytes were first purified from PBMC by a negative selection kit (Miltenyi Biotec, Auburn, CA) containing a cocktail of biotinylated anti- CD3, CD7, CD19, CD45RA and CD56 and immunoglobulin E (IgE) antibodies (Abs). By labeling with the primary antibody cocktail and secondary anti-biotin microbeads, non-monocyte populations including T cells, B cells, NK cells, granulocytes, dendritic cells and basophils were magnetized and trapped by the cell-sorting column (Miltenyi). The eluent fraction containing enriched monocytes was labeled with a microbead-conjugated anti-human CD14 Ab (Miltenyi) and purified through an additional positive selection. Monocytes were then allowed to attach to culture surfaces for 4h, followed by culture media washes until no floating cells observed.

The purity of monocytes was then determined by flow cytometry with fluorescent labeling of anti-human CD14, CD3 and CD4 Abs (Miltenyi), and analyzed by a FACSCalibur flow cytometer (Becton Dickinson, San Jose, CA). With this purification method, we can acquire monocytes with a purity of >99.9% with undetectable T cell contamination based on both flow cytometry and CD3 mRNA evaluations [15], [17], [20].

Purified monocytes from HIV-1 infected patients were allowed to differentiate for 3 d in Iscove’s medium (IMDM; Invitrogen, Carlsbad, CA) complete media containing 10% heat-activated AB+ human serum (Valley Biomedical, Winchester, VA), 1000 U/ml recombinant human macrophage colony-stimulating factor (rhMCSF; R&D Systems, Minneapolis, MN) and 1× penicillin/streptomycin (pen/strep; Invitrogen). Meanwhile, PBMC from healthy donors (HIV, HBV and STD negative; Puget Sound Blood Center, Seattle, WA) were subjected to CD8+ cell depletion using magnetic bead-conjugated anti-human CD8 Ab (Dynal, Oslo, Norway) and cultured in RPMI media (Invitrogen) supplemented with 15% fetal bovine serum (FBS) (Invitrogen), 1× pen/strep and 1 µg/ml phytohaemagglutinin (PHA; Remel Products, Lenexa, KS) for 2–3 d.

After 3 d of differentiation, patient MDM were co-cultivated with PHA stimulated and CD8-depleted donor PBMC in IMDM complete medium with no MCSF supplement. Co-cultures were maintained for 4 w with the addition of fresh PHA-stimulated, CD8-depleted donor PBMC every 3 d. The culture supernatants were collected every 3–4 d, and viral replication was monitored using an HIV-1 p24CA antigen capture assay kit (National Cancer Institute, Frederick, MD) following the manufacturer’s instructions. HIV-1 primary isolate expansions were titrated by Reed-Muench 50% tissue culture infectious dose (TCID50) assay.

Isolation of Infectious HIV-1 from Patient CD4+ T cells

Patient CD4+ T cells were purified from PBMC with a similar two-step strategy to that used for monocyte isolation. First, CD4+ T cells from study subjects were enriched using the CD4+ T cell Isolation Kit II (Miltenyi) according to the manufacturer’s instructions. Second, a positive selection using microbead-conjugated anti-human CD4 Ab (Miltenyi) was performed on the enriched CD4+ T cells. Purified patient CD4+ T cells were cultured in RPMI 1640 complete media supplemented with 100 U/ml IL-2 for 24 h, followed by co-cultivating with PHA-stimulated and CD8-depleted donor PBMC (donor PBMC to patient CD4+ T cell ratio of 2:1). Co-cultures were maintained for 1–4 w with the addition of fresh PHA-stimulated CD8-depleted donor PBMC every 3–4 d [45]. The culture supernatants were collected every 3–4 d, and viral replication was monitored using the HIV-1 p24CA antigen capture assay kit (NCI). The isolates were titrated by Reed and Muench TCID50 assay.

Co-receptor Usage Prediction

As positive or negative controls to validate indicator cell lines, HIV-1 laboratory-adapted strains including BaL, IIIB, ADA and SF2 were obtained from NIH AIDS Research and Reference Reagent Program; in addition, a known R5-tropic HIV-1 primary isolate acquired by our lab, 1192PB was used as a control virus. Co-receptor usage was predicted according to the V3 sequences of different isolates by employing the 11/25 rule [86], Geno2pheno (http://coreceptor.bioinf.mpi-inf.mpg.de/​index.php) [58] with a false-positive rate of 10%, and the Position-Specific Scoring Matrix (PSSM) approach (http://ubik.microbiol.washington.edu/com​puting/pssm/) [59].

Biological Confirmation of the Co-receptor Usage

Three U87 cell lines (NIH AIDS Research and Reference Reagent Program) were tested, including U87.CD4, U87.CD4.CXCR4 and U87.CD4.CCR5. Cells were thawed and passaged once before being seeded into 24-well plates at 1×104 cells/well, and incubated 6 h in complete DMEM containing 300 µg/ml G418 (Invitrogen). An additional 1 µg/ml of puromycin (Sigma-Aldrich, St Louis, MO) was supplemented in both U87.CD4.CXCR4 and U87.CD4.CCR5 media, but not in U87.CD4 media. Cells were infected with HIV-1 at MOI = 0.01 and HIV-1 p24 antigen production was monitored.

Three U373-MAGI (MAGI) cell lines (NIH AIDS Research and Reference Reagent Program) were tested, including MAGI.CD4, MAGI.CD4.CXCR4 and MAGI.CD4.CCR5. Cells were cultured in complete DMEM containing 0.2 mg/ml G418 and 0.1 mg/ml hygromycin B (Invitrogen), and MAGI.CD4.CXCR4 and MAGI.CD4.CCR5 cell cultures were additionally supplemented with 1.0 µg/ml puromycin. Cells were infected with HIV-1 at MOI = 0.01 and 5-bromo-4-chloro-3-indoyl-β-D-galactosid​e(X-gal; Sigma) staining was performed. Cells were observed using a Zeiss microscope, and images were acquired using the AxioVision software (Carl Zeiss, Jena, Germany).

Cyto-immunochemistry

The immune-detection of target molecules was performed as described previously [33]. Briefly, MDM were allowed to attach on cover glass while infection experiment performed. While staining, primary Abs used included mouse anti-human CD14 Ab, mouse-anti-HIV-1 p24 Ab (Dako, Carpenteria, CA); secondary fluorescence-conjugated Abs and DAPI-containing mounting solution were obtained from Invitrogen. Samples were observed with a Zeiss LSM 510 META NLO microscope (Zeiss, Thornwood, NY).

HIV-1 PCR and Sequencing

PCR primers and conditions for env C2-V3-C3 were described previously [15], [17], [20]. HIV-1 gag, polA (5′ half of the pol region) and polB (3′ half of the pol region), was also amplified from viral cDNA with nested PCR. Primers were designed according to the HIV-1 HXB2 sequence from HIV-1 Database (Los Alamos National Laboratories, Los Alamos, NM); they were: outer primers including PG1 (positions 790-814; 5′-atgggtgcgagagcgtcggtattaa-3′) and PG4 (positions 2408-2382; 5′- acctccaattccccctatcatttttgg-3′), as well as inner primers including PG7 (positions 880-902; 5′-ctaaaacatatagtatgggcaag-3′) and PG2 (positions 2357-2328; 5′- ttcttctaatactgtatcatctgctcctgt-3′). Primers for polA were: outer primers of POL3 (positions 2003–2029; 5′-gcagggcccctaggaaaaagggctgtt-3′) and P58 (positions 3800-3777; 5′-gacaaactcccactcaggaatcca-3′), as well as inner primers of POL1 (positions 2031–2057; 5′-gaaatgtggaaaggaaggacaccaaat-3′) and P56 (positions 3758-3725; 5′-tgtccaccatgcttcccatgtttccttttgtatg-3′​).Primers for polB were: outer primers of POL9 (positions 3425–3450; 5′-aataccactaacagaagaagcagagc-3′) and POL8 (5350-5325; 5′-ctgctaggtcagggtctacttgtgtg-3′), as well as inner primers of POL7 (positions 3528–3553; 5′-gcagaaatacagaagcaggggcaagg-3′) and POL6 (positions 5220-5195; 5′-ccctagtgggatgtgtacttctgaac-3′). HIV copy numbers were calculated based on limiting-dilution PCR with the QUALITY program as previously described [61]. HIV-1 sequences diversity was calculated using the HKY85 evolutionary model with the program DIVEIN [87].

Statistical Analysis

Data were analyzed for statistical significance by two-tailed Student’s t-test, one-way or two-way ANOVA with Student post hoc test using GraphPad Prism version 5.02 (GraphPad Software, Inc., San Diego, CA), or by GEE analysis by employing the “pwr” package for R (http://cran.r-project.org/web/packages/p​wr/index.html). P<0.05 was deemed significant.

Acknowledgments

We thank Professor James Mullins, Carrie K. Wilcox and Victor Swain, University of Washington for their great assistance on the virological technologies.

Author Contributions

Conceived and designed the experiments: TZ TW. Performed the experiments: TW YX HZ TA SBI CP JD GCD DF. Analyzed the data: TW HZ SBI MZ ZY SH LC. Wrote the paper: TW TZ YX.

References

  1. 1. Muller WA, Randolph GJ (1999) Migration of leukocytes across endothelium and beyond: molecules involved in the transmigration and fate of monocytes. J Leukoc Biol 66: 698–704.
  2. 2. Randolph GJ, Sanchez-Schmitz G, Liebman RM, Schakel K (2002) The CD16(+) (FcgammaRIII(+)) subset of human monocytes preferentially becomes migratory dendritic cells in a model tissue setting. J Exp Med 196: 517–527. doi: 10.1084/jem.20011608
  3. 3. Wiley CA, Schrier RD, Nelson JA, Lampert PW, Oldstone MB (1986) Cellular localization of human immunodeficiency virus infection within the brains of acquired immune deficiency syndrome patients. Proc Natl Acad Sci U S A 83: 7089–7093. doi: 10.1073/pnas.83.18.7089
  4. 4. Ho DD, Rota TR, Hirsch MS (1986) Infection of monocyte/macrophages by human T lymphotropic virus type III. J Clin Invest 77: 1712–1715. doi: 10.1172/jci112491
  5. 5. Schnittman SM, Lane HC, Greenhouse J, Justement JS, Baseler M, et al. (1990) Preferential infection of CD4+ memory T cells by human immunodeficiency virus type 1: evidence for a role in the selective T-cell functional defects observed in infected individuals. Proc Natl Acad Sci U S A 87: 6058–6062. doi: 10.1073/pnas.87.16.6058
  6. 6. Fox CH, Tenner-Racz K, Racz P, Firpo A, Pizzo PA, et al. (1991) Lymphoid germinal centers are reservoirs of human immunodeficiency virus type 1 RNA. J Infect Dis 164: 1051–1057. doi: 10.1093/infdis/164.6.1051
  7. 7. Embretson J, Zupancic M, Ribas JL, Burke A, Racz P, et al. (1993) Massive covert infection of helper T lymphocytes and macrophages by HIV during the incubation period of AIDS. Nature 362: 359–362. doi: 10.1038/362359a0
  8. 8. Pantaleo G, Graziosi C, Demarest JF, Butini L, Montroni M, et al. (1993) HIV infection is active and progressive in lymphoid tissue during the clinically latent stage of disease. Nature 362: 355–358. doi: 10.1038/362355a0
  9. 9. Sonza S, Maerz A, Deacon N, Meanger J, Mills J, et al. (1996) Human immunodeficiency virus type 1 replication is blocked prior to reverse transcription and integration in freshly isolated peripheral blood monocytes. J Virol 70: 3863–3869.
  10. 10. Orenstein JM, Fox C, Wahl SM (1997) Macrophages as a source of HIV during opportunistic infections. Science 276: 1857–1861. doi: 10.1126/science.276.5320.1857
  11. 11. Cavert W, Notermans DW, Staskus K, Wietgrefe SW, Zupancic M, et al. (1997) Kinetics of response in lymphoid tissues to antiretroviral therapy of HIV-1 infection. Science 276: 960–964. doi: 10.1126/science.276.5314.960
  12. 12. Schrager LK, D’Souza MP (1998) Cellular and anatomical reservoirs of HIV-1 in patients receiving potent antiretroviral combination therapy. JAMA 280: 67–71. doi: 10.1001/jama.280.1.67
  13. 13. Cavert W, Haase AT (1998) A national tissue bank to track HIV eradication and immune reconstruction. Science 280: 1865–1866. doi: 10.1126/science.280.5371.1865
  14. 14. Veazey RS, DeMaria M, Chalifoux LV, Shvetz DE, Pauley DR, et al. (1998) Gastrointestinal tract as a major site of CD4+ T cell depletion and viral replication in SIV infection. Science 280: 427–431. doi: 10.1126/science.280.5362.427
  15. 15. Fulcher JA, Hwangbo Y, Zioni R, Nickle D, Lin X, et al. (2004) Compartmentalization of human immunodeficiency virus type 1 between blood monocytes and CD4+ T cells during infection. J Virol 78: 7883–7893. doi: 10.1128/jvi.78.15.7883-7893.2004
  16. 16. Delobel P, Sandres-Saune K, Cazabat M, L’Faqihi FE, Aquilina C, et al. (2005) Persistence of distinct HIV-1 populations in blood monocytes and naive and memory CD4 T cells during prolonged suppressive HAART. AIDS 19: 1739–1750. doi: 10.1097/01.aids.0000183125.93958.26
  17. 17. Llewellyn N, Zioni R, Zhu H, Andrus T, Xu Y, et al. (2006) Continued evolution of HIV-1 circulating in blood monocytes with antiretroviral therapy: genetic analysis of HIV-1 in monocytes and CD4+ T cells of patients with discontinued therapy. J Leukoc Biol 80: 1118–1126. doi: 10.1189/jlb.0306144
  18. 18. Xu Y, Zhu H, Wilcox CK, van’t Wout A, Andrus T, et al. (2008) Blood monocytes harbor HIV type 1 strains with diversified phenotypes including macrophage-specific CCR5 virus. J Infect Dis 197: 309–318. doi: 10.1086/524847
  19. 19. Zhu T (2002) HIV-1 in peripheral blood monocytes: an underrated viral source. J Antimicrob Chemother 50: 309–311. doi: 10.1093/jac/dkf143
  20. 20. Zhu T, Muthui D, Holte S, Nickle D, Feng F, et al. (2002) Evidence for human immunodeficiency virus type 1 replication in vivo in CD14(+) monocytes and its potential role as a source of virus in patients on highly active antiretroviral therapy. J Virol 76: 707–716. doi: 10.1128/jvi.76.2.707-716.2002
  21. 21. Valcour VG, Shiramizu BT, Sithinamsuwan P, Nidhinandana S, Ratto-Kim S, et al. (2009) HIV DNA and cognition in a Thai longitudinal HAART initiation cohort: the SEARCH 001 Cohort Study. Neurology 72: 992–998. doi: 10.1212/01.wnl.0000344404.12759.83
  22. 22. Crowe SM, Westhorpe CL, Mukhamedova N, Jaworowski A, Sviridov D, et al. (2010) The macrophage: the intersection between HIV infection and atherosclerosis. J Leukoc Biol 87: 589–598. doi: 10.1189/jlb.0809580
  23. 23. Persidsky Y (1999) Model systems for studies of leukocyte migration across the blood - brain barrier. J Neurovirol 5: 579–590. doi: 10.3109/13550289909021287
  24. 24. Persidsky Y, Heilman D, Haorah J, Zelivyanskaya M, Persidsky R, et al. (2006) Rho-mediated regulation of tight junctions during monocyte migration across the blood-brain barrier in HIV-1 encephalitis (HIVE). Blood 107: 4770–4780. doi: 10.1182/blood-2005-11-4721
  25. 25. Ramirez SH, Heilman D, Morsey B, Potula R, Haorah J, et al. (2008) Activation of peroxisome proliferator-activated receptor gamma (PPARgamma) suppresses Rho GTPases in human brain microvascular endothelial cells and inhibits adhesion and transendothelial migration of HIV-1 infected monocytes. J Immunol 180: 1854–1865. doi: 10.4049/jimmunol.180.3.1854
  26. 26. Gendelman HE, Ding S, Gong N, Liu J, Ramirez SH, et al. (2009) Monocyte chemotactic protein-1 regulates voltage-gated K+ channels and macrophage transmigration. J Neuroimmune Pharmacol 4: 47–59. doi: 10.1007/s11481-008-9135-1
  27. 27. Westhorpe CL, Zhou J, Webster NL, Kalionis B, Lewin SR, et al. (2009) Effects of HIV-1 infection in vitro on transendothelial migration by monocytes and monocyte-derived macrophages. J Leukoc Biol 85: 1027–1035. doi: 10.1189/jlb.0808501
  28. 28. Gonzalez-Scarano F, Martin-Garcia J (2005) The neuropathogenesis of AIDS. Nat Rev Immunol 5: 69–81. doi: 10.1038/nri1527
  29. 29. Ghafouri M, Amini S, Khalili K, Sawaya BE (2006) HIV-1 associated dementia: symptoms and causes. Retrovirology 3: 28. doi: 10.1186/1742-4690-3-28
  30. 30. Aquaro S, Svicher V, Ronga L, Perno CF, Pollicita M (2008) HIV-1-associated dementia during HAART therapy. Recent Patents CNS Drug Discov 3: 23–33. doi: 10.2174/157488908783421438
  31. 31. Marsden MD, Zack JA (2009) Eradication of HIV: current challenges and new directions. J Antimicrob Chemother 63: 7–10. doi: 10.1093/jac/dkn455
  32. 32. Persidsky Y, Stins M, Way D, Witte MH, Weinand M, et al. (1997) A model for monocyte migration through the blood-brain barrier during HIV-1 encephalitis. J Immunol 158: 3499–3510. doi: 10.1016/s0002-9440(10)65476-4
  33. 33. Wang T, Gong N, Liu J, Kadiu I, Kraft-Terry SD, et al. (2008) Proteomic modeling for HIV-1 infected microglia-astrocyte crosstalk. PLoS ONE 3: e2507. doi: 10.1371/journal.pone.0002507
  34. 34. Wang T, Gong N, Liu J, Kadiu I, Kraft-Terry SD, et al. (2008) HIV-1-infected astrocytes and the microglial proteome. J Neuroimmune Pharmacol 3: 173–186. doi: 10.1007/s11481-008-9110-x
  35. 35. Chaudhuri A, Yang B, Gendelman HE, Persidsky Y, Kanmogne GD (2008) STAT1 signaling modulates HIV-1-induced inflammatory responses and leukocyte transmigration across the blood-brain barrier. Blood 111: 2062–2072. doi: 10.1182/blood-2007-05-091207
  36. 36. Kelly J, Beddall MH, Yu D, Iyer SR, Marsh JW, et al. (2008) Human macrophages support persistent transcription from unintegrated HIV-1 DNA. Virology 372: 300–312. doi: 10.1016/j.virol.2007.11.007
  37. 37. Valcour VG, Shiramizu BT, Shikuma CM (2010) HIV DNA in circulating monocytes as a mechanism to dementia and other HIV complications. J Leukoc Biol 87: 621–626. doi: 10.1189/jlb.0809571
  38. 38. Lambotte O, Taoufik Y, de Goer MG, Wallon C, Goujard C, et al. (2000) Detection of infectious HIV in circulating monocytes from patients on prolonged highly active antiretroviral therapy. J Acquir Immune Defic Syndr 23: 114–119. doi: 10.1097/00126334-200002010-00002
  39. 39. Sonza S, Mutimer HP, Oelrichs R, Jardine D, Harvey K, et al. (2001) Monocytes harbour replication-competent, non-latent HIV-1 in patients on highly active antiretroviral therapy. AIDS 15: 17–22. doi: 10.1097/00002030-200101050-00005
  40. 40. Ho DD, Neumann AU, Perelson AS, Chen W, Leonard JM, et al. (1995) Rapid turnover of plasma virions and CD4 lymphocytes in HIV-1 infection. Nature 373: 123–126. doi: 10.1038/373123a0
  41. 41. Wei X, Ghosh SK, Taylor ME, Johnson VA, Emini EA, et al. (1995) Viral dynamics in human immunodeficiency virus type 1 infection. Nature 373: 117–122. doi: 10.1038/373117a0
  42. 42. Perelson AS, Neumann AU, Markowitz M, Leonard JM, Ho DD (1996) HIV-1 dynamics in vivo: virion clearance rate, infected cell life-span, and viral generation time. Science 271: 1582–1586. doi: 10.1126/science.271.5255.1582
  43. 43. Finzi D, Hermankova M, Pierson T, Carruth LM, Buck C, et al. (1997) Identification of a reservoir for HIV-1 in patients on highly active antiretroviral therapy. Science 278: 1295–1300. doi: 10.1126/science.278.5341.1295
  44. 44. Chun TW, Stuyver L, Mizell SB, Ehler LA, Mican JA, et al. (1997) Presence of an inducible HIV-1 latent reservoir during highly active antiretroviral therapy. Proc Natl Acad Sci U S A 94: 13193–13197. doi: 10.1073/pnas.94.24.13193
  45. 45. Chun TW, Engel D, Berrey MM, Shea T, Corey L, et al. (1998) Early establishment of a pool of latently infected, resting CD4(+) T cells during primary HIV-1 infection. Proc Natl Acad Sci U S A 95: 8869–8873. doi: 10.1073/pnas.95.15.8869
  46. 46. Finzi D, Blankson J, Siliciano JD, Margolick JB, Chadwick K, et al. (1999) Latent infection of CD4+ T cells provides a mechanism for lifelong persistence of HIV-1, even in patients on effective combination therapy. Nat Med 5: 512–517.
  47. 47. Natarajan V, Bosche M, Metcalf JA, Ward DJ, Lane HC, et al. (1999) HIV-1 replication in patients with undetectable plasma virus receiving HAART. Highly active antiretroviral therapy [letter]. Lancet 353: 119–120. doi: 10.1016/s0140-6736(05)76156-0
  48. 48. Zhang ZQ, Schuler T, Cavert W, Notermans DW, Gebhard K, et al. (1999) Reversibility of the pathological changes in the follicular dendritic cell network with treatment of HIV-1 infection. Proc Natl Acad Sci U S A 96: 5169–5172. doi: 10.1073/pnas.96.9.5169
  49. 49. Furtado MR, Callaway DS, Phair JP, Kunstman KJ, Stanton JL, et al. (1999) Persistence of HIV-1 transcription in peripheral-blood mononuclear cells in patients receiving potent antiretroviral therapy [see comments]. N Engl J Med 340: 1614–1622. doi: 10.1056/nejm199905273402102
  50. 50. Chun TW, Davey RT Jr, Ostrowski M, Shawn Justement J, Engel D, et al. (2000) Relationship between pre-existing viral reservoirs and the re-emergence of plasma viremia after discontinuation of highly active anti-retroviral therapy. Nat Med 6: 757–761.
  51. 51. Sharkey ME, Teo I, Greenough T, Sharova N, Luzuriaga K, et al. (2000) Persistence of episomal HIV-1 infection intermediates in patients on highly active anti-retroviral therapy. Nat Med 6: 76–81.
  52. 52. Bailey JR, Sedaghat AR, Kieffer T, Brennan T, Lee PK, et al. (2006) Residual human immunodeficiency virus type 1 viremia in some patients on antiretroviral therapy is dominated by a small number of invariant clones rarely found in circulating CD4+ T cells. J Virol 80: 6441–6457. doi: 10.1128/jvi.00591-06
  53. 53. Zhu T (2000) HIV-1 genotypes in peripheral blood monocytes. J Leukoc Biol 68: 338–344.
  54. 54. Crowe S, Zhu T, Muller WA (2003) The contribution of monocyte infection and trafficking to viral persistence, and maintenance of the viral reservoir in HIV infection. J Leukoc Biol 74: 635–641. doi: 10.1189/jlb.0503204
  55. 55. Schacker T, Collier AC, Hughes J, Shea T, Corey L (1996) Clinical and epidemiologic features of primary HIV infection. Ann Intern Med 125: 257–264. doi: 10.7326/0003-4819-125-4-199608150-00001
  56. 56. Schacker TW, Hughes JP, Shea T, Coombs RW, Corey L (1998) Biological and virologic characteristics of primary HIV infection. Ann Intern Med 128: 613–620. doi: 10.7326/0003-4819-128-8-199804150-00001
  57. 57. Resch W, Hoffman N, Swanstrom R (2001) Improved success of phenotype prediction of the human immunodeficiency virus type 1 from envelope variable loop 3 sequence using neural networks. Virology 288: 51–62. doi: 10.1006/viro.2001.1087
  58. 58. Beerenwinkel N, Daumer M, Oette M, Korn K, Hoffmann D, et al. (2003) Geno2pheno: Estimating phenotypic drug resistance from HIV-1 genotypes. Nucleic Acids Res 31: 3850–3855. doi: 10.1093/nar/gkg575
  59. 59. Jensen MA, Li FS, van’t Wout AB, Nickle DC, Shriner D, et al. (2003) Improved coreceptor usage prediction and genotypic monitoring of R5-to-X4 transition by motif analysis of human immunodeficiency virus type 1 env V3 loop sequences. J Virol 77: 13376–13388. doi: 10.1128/jvi.77.24.13376-13388.2003
  60. 60. Graham SM, Holte S, Kimata JT, Wener MH, Overbaugh J (2009) A decrease in albumin in early SIV infection is related to viral pathogenicity. AIDS Res Hum Retroviruses 25: 433–440. doi: 10.1089/aid.2008.0267
  61. 61. Zhu T, Corey L, Hwangbo Y, Lee JM, Learn GH, et al. (2003) Persistence of extraordinarily low levels of genetically homogeneous human immunodeficiency virus type 1 in exposed seronegative individuals. J Virol 77: 6108–6116. doi: 10.1128/jvi.77.11.6108-6116.2003
  62. 62. Aquaro S, Perno CF, Balestra E, Balzarini J, Cenci A, et al. (1997) Inhibition of replication of HIV in primary monocyte/macrophages by different antiviral drugs and comparative efficacy in lymphocytes. J Leukoc Biol 62: 138–143.
  63. 63. Perno CF, Newcomb FM, Davis DA, Aquaro S, Humphrey RW, et al. (1998) Relative potency of protease inhibitors in monocytes/macrophages acutely and chronically infected with human immunodeficiency virus. J Infect Dis 178: 413–422. doi: 10.1086/515642
  64. 64. Aquaro S, Menten P, Struyf S, Proost P, Van Damme J, et al. (2001) The LD78beta isoform of MIP-1alpha is the most potent CC-chemokine in inhibiting CCR5-dependent human immunodeficiency virus type 1 replication in human macrophages. J Virol 75: 4402–4406. doi: 10.1128/jvi.75.9.4402-4406.2001
  65. 65. Aquaro S, Bagnarelli P, Guenci T, De Luca A, Clementi M, et al. (2002) Long-term survival and virus production in human primary macrophages infected by human immunodeficiency virus. J Med Virol 68: 479–488. doi: 10.1002/jmv.10245
  66. 66. Carter CC, Onafuwa-Nuga A, McNamara LA, Riddell Jt, Bixby D, et al. (2010) HIV-1 infects multipotent progenitor cells causing cell death and establishing latent cellular reservoirs. Nat Med 16: 446–451. doi: 10.1038/nm.2109
  67. 67. Kadiu I, Narayanasamy P, Dash PK, Zhang W, Gendelman HE (2012) Biochemical and biologic characterization of exosomes and microvesicles as facilitators of HIV-1 infection in macrophages. J Immunol 189: 744–754. doi: 10.4049/jimmunol.1102244
  68. 68. Tuttle DL, Anders CB, Aquino-De Jesus MJ, Poole PP, Lamers SL, et al. (2002) Increased replication of non-syncytium-inducing HIV type 1 isolates in monocyte-derived macrophages is linked to advanced disease in infected children. AIDS Res Hum Retroviruses 18: 353–362. doi: 10.1089/088922202753519133
  69. 69. Gray L, Sterjovski J, Churchill M, Ellery P, Nasr N, et al. (2005) Uncoupling coreceptor usage of human immunodeficiency virus type 1 (HIV-1) from macrophage tropism reveals biological properties of CCR5-restricted HIV-1 isolates from patients with acquired immunodeficiency syndrome. Virology 337: 384–398. doi: 10.1016/j.virol.2005.04.034
  70. 70. Yi Y, Rana S, Turner JD, Gaddis N, Collman RG (1998) CXCR-4 is expressed by primary macrophages and supports CCR5-independent infection by dual-tropic but not T-tropic isolates of human immunodeficiency virus type 1. J Virol 72: 772–777.
  71. 71. Yi Y, Shaheen F, Collman RG (2005) Preferential use of CXCR4 by R5X4 human immunodeficiency virus type 1 isolates for infection of primary lymphocytes. J Virol 79: 1480–1486. doi: 10.1128/jvi.79.3.1480-1486.2005
  72. 72. Triques K, Stevenson M (2004) Characterization of restrictions to human immunodeficiency virus type 1 infection of monocytes. J Virol 78: 5523–5527. doi: 10.1128/jvi.78.10.5523-5527.2004
  73. 73. Arfi V, Riviere L, Jarrosson-Wuilleme L, Goujon C, Rigal D, et al. (2008) Characterization of the early steps of infection of primary blood monocytes by human immunodeficiency virus type 1. J Virol 82: 6557–6565. doi: 10.1128/jvi.02321-07
  74. 74. Cywin CL, Klunder JM, Hoermann M, Brickwood JR, David E, et al. (1998) Novel nonnucleoside inhibitors of HIV-1 reverse transcriptase. 8. 8-Aryloxymethyl- and 8-arylthiomethyldipyridodiazepinones. J Med Chem 41: 2972–2984. doi: 10.1021/jm9707030
  75. 75. Uhlmann EJ, Tebas P, Storch GA, Powderly WG, Lie YS, et al. (2004) Effects of the G190A substitution of HIV reverse transcriptase on phenotypic susceptibility of patient isolates to delavirdine. J Clin Virol 31: 198–203. doi: 10.1016/j.jcv.2004.03.012
  76. 76. Wind-Rotolo M, Durand C, Cranmer L, Reid A, Martinson N, et al. (2009) Identification of nevirapine-resistant HIV-1 in the latent reservoir after single-dose nevirapine to prevent mother-to-child transmission of HIV-1. J Infect Dis 199: 1301–1309. doi: 10.1086/597759
  77. 77. Kagan RM, Sista P, Pattery T, Bacheler L, Schwab DA (2009) Additional HIV-1 mutation patterns associated with reduced phenotypic susceptibility to etravirine in clinical samples. AIDS 23: 1602–1605. doi: 10.1097/qad.0b013e32832d8771
  78. 78. Soulie C, Assoumou L, Ghosn J, Duvivier C, Peytavin G, et al. (2009) Nucleoside reverse transcriptase inhibitor-sparing regimen (nonnucleoside reverse transcriptase inhibitor+protease inhibitor) was more likely associated with resistance comparing to nonnucleoside reverse transcriptase inhibitor or protease inhibitor+nucleoside reverse transcriptase inhibitor in the randomized ANRS 121 trial. Aids 23: 1605–1608. doi: 10.1097/qad.0b013e32832d9031
  79. 79. Polilli E, Di Masi F, Sozio F, Mazzotta E, Alterio L, et al. (2009) Sequential transmission and long-term persistence of an HIV strain partially resistant to protease inhibitors. New Microbiol 32: 205–208.
  80. 80. O’Brien WA, Namazi A, Kalhor H, Mao SH, Zack JA, et al. (1994) Kinetics of human immunodeficiency virus type 1 reverse transcription in blood mononuclear phagocytes are slowed by limitations of nucleotide precursors. J Virol 68: 1258–1263.
  81. 81. Bergamaschi A, Pancino G (2010) Host hindrance to HIV-1 replication in monocytes and macrophages. Retrovirology 7: 31. doi: 10.1186/1742-4690-7-31
  82. 82. Peng G, Greenwell-Wild T, Nares S, Jin W, Lei KJ, et al. (2007) Myeloid differentiation and susceptibility to HIV-1 are linked to APOBEC3 expression. Blood 110: 393–400. doi: 10.1182/blood-2006-10-051763
  83. 83. Bishop KN, Verma M, Kim EY, Wolinsky SM, Malim MH (2008) APOBEC3G inhibits elongation of HIV-1 reverse transcripts. PLoS Pathog 4: e1000231. doi: 10.1371/journal.ppat.1000231
  84. 84. Laguette N, Sobhian B, Casartelli N, Ringeard M, Chable-Bessia C, et al. (2011) SAMHD1 is the dendritic- and myeloid-cell-specific HIV-1 restriction factor counteracted by Vpx. Nature 474: 654–657. doi: 10.1038/nature10117
  85. 85. Hrecka K, Hao C, Gierszewska M, Swanson SK, Kesik-Brodacka M, et al. (2011) Vpx relieves inhibition of HIV-1 infection of macrophages mediated by the SAMHD1 protein. Nature 474: 658–661. doi: 10.1038/nature10195
  86. 86. De Jong JJ, De Ronde A, Keulen W, Tersmette M, Goudsmit J (1992) Minimal requirements for the human immunodeficiency virus type 1 V3 domain to support the syncytium-inducing phenotype: analysis by single amino acid substitution. J Virol 66: 6777–6780.
  87. 87. Deng W, Maust BS, Nickle DC, Learn GH, Liu Y, et al. (2010) DIVEIN: a web server to analyze phylogenies, sequence divergence, diversity, and informative sites. BioTechniques 48: 405–408. doi: 10.2144/000113370