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HIV cure efforts are hampered by limited characterization of the cells supporting HIV replication in vivo and inadequate methods for quantifying the latent viral reservoir in patients receiving antiretroviral therapy. We combine fluorescent in situ RNA hybridization with detection of HIV protein and flow cytometry, enabling detection of 0.5–1 gag-pol mRNA+/Gag protein+ infected cells per million. In the peripheral blood of untreated persons, active HIV replication correlated with viremia, and occurred in CD4 T cells expressing T follicular helper cell markers and inhibitory co-receptors. In virally-suppressed subjects, the approach identified latently infected cells capable of producing HIV mRNA and protein after stimulation with PMA/ionomycin and latency-reversing agents (LRAs). While ingenol-induced reactivation mirrored the effector and central/transitional memory CD4 T cell contribution to the pool of integrated HIV DNA, bryostatin-induced reactivation occurred predominantly in cells expressing effector memory markers. This indicates that CD4 T cell differentiation status differentially affects LRA effectiveness.
Technological limitations hamper characterization of CD4 T cells supporting ongoing HIV infection and quantification of the latent reservoir. Baxter, et al. use simultaneous detection of viral protein and mRNA to quantify and phenotype both the ongoing infection during viremia and the translation-competent inducible reservoir in virally-supressed, treated patients.
More than three decades after the identification of CD4 T lymphocytes as the main target of human immunodeficiency virus (HIV) infection, surprisingly little is still known about the characteristics of cells that support HIV replication in vivo (Swanstrom and Coffin, 2012) and serve as long-lived viral reservoirs in ART-treated individuals (Kulpa and Chomont, 2015). A deeper understanding of the frequency, phenotype and regulation of these cells is critical for the development of targeted HIV cure strategies and vaccines eliciting immune responses capable of eliminating early foci of infection (Burton et al., 2012). Furthermore, determination of the tissue and cellular sources of persistent virus and the development of high-throughput scalable assays to measure the latent reservoir in patients have both been identified as key priorities in HIV eradication research (Deeks et al., 2012). This critical need is demonstrated by the focusing of cure efforts on latency-reversing agents (LRAs) even though their relative ability to induce latently infected cells of different phenotypes and differentiation states is not known.
To accurately measure in vivo the frequency and phenotype of CD4 T cells producing viral proteins, we developed a highly sensitive flow cytometry assay enabling simultaneous assessment of HIV RNA and Gag proteins, along with quantitation of phenotypic CD4 T cell molecules. We applied this technology to perform single-cell analysis of CD4 T cells harboring spontaneously produced and activation-inducible virus in treated and untreated individuals, quantitate viral reservoirs and define the frequency and phenotype of primary CD4 T cells from patient blood that could be induced from latency.
Current flow cytometry methods are not sensitive or specific enough to assess HIV-infected cells in patient samples. We thus explored the capacity of fluorescent in situ hybridization for gene-specific mRNA (mRNA flow-FISH) to detect HIV transcription in infected CD4 T cells (Porichis et al., 2014). In this approach, multiple oligomeric probes and branched DNA signal amplification enhance detection sensitivity (Figure S1). We selected combined probe sets against the gag and pol genes as their sequences are well conserved across clinical isolates and they are the most abundant viral transcripts in samples from both treated and untreated patients (Bagnarelli et al., 1996). See Table S1 for sequences used in probe design. Robust mRNA staining was detected in a primary CD4 T cell culture from an HIV-infected individual after expansion of endogenous virus (Figure 1A). Combining this method with staining for HIV protein using the Gag-specific KC57 antibody allowed for concurrent detection of HIV transcription and translation products. We could readily detect double positive (HIVRNA+/Gag+) cells in the expanded culture. This population was abrogated by addition of antiviral drugs to the culture and was not present in T cells from uninfected control (UC) donors cultured and processed in parallel (Figure 1B). We define this population of HIVRNA+/Gag+ cells as viral translation-competent, as the cells detected contain virus capable of producing HIV mRNA and proteins.
To determine the specificity and linearity of this HIVRNA/Gag assay, we spiked expanded HIV-replicating primary CD4 T cells into uninfected CD4. HIV RNA/protein co-staining showed excellent consistency down to the lowest dilutions tested (23/million, R2=0.9996, Figures 1CD, 1/million, R2=0.9856, Figures S2A–B). In contrast, background staining prevented reliable identification of infected cells for frequencies below 0.05–0.1%, the equivalent of 500–1000 HIVGag+ or HIVRNA+ T cells per million CD4, when we assessed a single marker (Figures 1EF, S2CD).
To verify that HIVRNA+/Gag+ cells were HIV-infected we sorted expanded HIV-infected CD4 T cells into HIV mRNA-negative/Gag protein-negative (HIVneg/neg) and HIVRNA+/Gag+ populations (Figure S2E) and subsequently measured integrated HIV DNA. The HIVRNA+/Gag+ subset was enriched for HIV DNA as compared to the HIVneg/neg population (Figure S2F), confirming that the HIVRNA/Gag assay identifies HIV-infected cells.
We next used confocal microscopy to determine whether this approach could provide semi-quantitative information about viral replication (Figures 1G–I). We expanded primary CD4 T cells isolated from one UC subject and two HIV-infected individuals (one untreated, one ART-treated). We then sorted cell subsets defined by HIV mRNA/protein expression patterns for imaging (Figure 1G, Figures S2G, S3A–C). Spot counting for gag-pol mRNA FISH signals revealed a low background in both the UC subject and the HIVneg/neg subset and clear signals in the three HIVRNA+ populations (Figure 1H, Figure S2H). Based on the false positive rate observed in the UC patient (Figure S2H), we determined a conservative detection limit to minimize false-positive events (assuming Gaussian distribution, mean+3SD) of 20 gag-pol mRNA spots per cell. This accounts for 93% of all HIVRNA+ cells (Figure S2H). The hierarchy of total gag-pol mRNA spot counts was consistent with flow cytometry MFIs of the sorted populations, with the HIVRNAbright/Gagbright cells harboring most spots (Figure 1H). As the intensity of individual spots will contribute to the global signal intensity of a given cell, we examined the total intensity of gag-pol mRNA signal for individual cells using corrected total cell fluorescence (CTCF) (Burgess et al., 2010). Again, we found a direct relationship to flow cytometry data (Figures S3D–H).
We measured the relative distribution of gag-pol RNA spots in the nuclear and cytoplasmic compartments amongst the sorted subsets. In HIVRNA+/Gag− cells, the vast majority of the gag-pol RNA spots were located in the nucleus and only a small fraction (median 5.1%) in the cytoplasm, whereas this proportion reached 30–40% in subsets also expressing Gag protein (Figure 1I). Such differences in localization were confirmed by Z-stack imaging (Movies S1–2). This is consistent with data suggesting that viral transcription leads to accumulation of gag-pol mRNA in the nucleus before its egress to the cytoplasm is enabled by Rev-mediated export (Karn and Stoltzfus, 2012). Although this assay is not designed for single molecule FISH, we demonstrate that it can be used semi-quantitatively to assess HIV transcription at the single-cell level. When used sequentially in flow sorting and confocal microscopy, it can greatly facilitate FISH studies of rare cell subsets of interest in heterogeneous populations.
Having validated the assay on infected CD4 T cells expanded in vitro, we next sought to determine the frequency of cells that produce HIV at a given time in the peripheral blood of subjects with untreated HIV infection (UNT), compared to UC donors (subject characteristics and number of cells analyzed: Table S2). We quantified in parallel the population that spontaneously produces viral mRNA and proteins and the additional cells that can be induced to express such viral markers after short-term 12 hr PMA/ionomycin (PMA/iono) stimulation. Whereas false positive events were very rare in UC (one HIVRNA+/Gag+ cell detected from 8 samples/7.7 million cells), we readily detected HIVRNA+/Gag+ CD4 in UNT subjects (median[range]=123[1.5–230]/per million CD4) (Figures 2AB), which were further increased upon stimulation with PMA/iono (median[range]=311[3.6–768]/million). The impact of PMA/iono was similar amongst subjects (Figure 2C, Figure S4A). This suggested that, besides CD4 T cells spontaneously producing viral proteins, an additional larger pool of infected lymphocytes appeared poised for rapid induction of viral transcription and translation upon stimulation in UNT individuals. The superiority of the RNA/protein co-staining method over single marker use was clear when we compared unstimulated, primary samples of UC to UNT donors (Figure 2D). The limit of HIVRNA+/Gag+ cell detection based on the UC false positive detection rate was 0.5–1/million, whereas high background staining rendered single KC57 Gag or mRNA staining alone non-interpretable in the 0–1000 cells/million range, the frequency bracket that contained all UNT subjects examined. This represents a gain in detection of 1000-fold over standard protein staining for HIV Gag.
We next assessed the correlation of HIVRNA+/Gag+ frequencies with markers of disease progression. There was a strong correlation with viral load in both the resting and PMA/iono stimulated conditions (Figure 2E, Figure S4C) and non-significant inverse correlations with CD4 count (Figure 2F, Figure S4B). Interestingly, we found the strongest correlations between the absolute number of HIV-infected cells per μL and viral load (Figure 2G). We also observed an increase in the gag-pol mRNA and Gag protein MFI on HIVRNA+/Gag+ cells following stimulation, suggesting increased viral production per cell when compared to spontaneous viral production (Figure S4DE). We confirmed the reproducibility of the assay across different experiments, flow panels and operators, even at lower frequencies of HIVRNA+/Gag+ CD4 (Figure S4F). Therefore, CD4 T cells that produce HIV RNAs and protein, either spontaneously ex vivo or after stimulation, can be reliably identified and quantified in primary clinical samples from subjects with progressive HIV infection.
The features of cells harboring replicating virus have thus far been largely inferred from in vitro infection or amplification of autologous virus, due to an inability to detect infected cells ex vivo using previously applied methods. To address this, we assessed the phenotype of HIVRNA+/Gag+ CD4 T cells in primary UNT samples, analyzed directly from leukapheresis donation and without additional ex vivo stimulation. Such cells are defined here as in vivo infected. CD4 down-regulation is a hallmark of HIV infection in vitro, facilitating Env incorporation and viral replication (Arganaraz et al., 2003). We found that CD4 expression was profoundly diminished on in vivo infected HIVRNA+/Gag+ cells (Figures 3A–C), consistent with previous data (DeMaster et al., 2015). HLA-Class I downregulation, another well-known effect of Nef protein (Schwartz et al., 1996) was also observed in primary samples (Figure 3D), albeit at a more modest level than after stimulation and virus propagation ex vivo (Figure 3E). In contrast, HLA-Class II expression on in vivo infected cells differed from in vitro data; consistent with an activated state, HLA-DR was preferentially expressed on HIVRNA+/Gag+ compared to HIVRNA−/Gag− cells in primary samples (Figure 3F), whereas no enrichment for HIV-infected cells in the HLA-DR+ population was observed at days 5 and 7 of endogenous viral reactivation (Figure 3G). Differences were also observed for PD-L1 expression on HIVRNA+/Gag+ (Figures S5AB). Whereas PD-L1 was highly expressed on stimulated HIV-infected and non-infected cells early after initiation (e.g., day 3) of T cell cultures, suggesting a potential mechanism of functional immune escape similar to that described for cancer cells, PD-L1 expression was low on in vivo infected HIVRNA+/Gag+ CD4. The latter was surprising given the same cells preferentially expressed HLA-DR, another marker of activation. Thus, the phenotype of HIV-replicating cells in vivo cannot be reliably inferred from in vitro expansion models.
Central memory cells are major long-lived viral reservoirs in ART-treated subjects (Chomont et al., 2009). However, whether viral replication during viremia preferentially occurs in this subset remains to be defined. We analyzed the differentiation of HIVRNA+/Gag+ CD4 T cells according to CD45RA and CD27 expression (Figure 3H), described here as naive (Tnaive: CD27+ CD45RA+), central/transitional memory (TCM/TM: CD27+ CD45RA−), effector memory (TEM: CD27− CD45RA−) and terminally differentiated (TTD: CD27− CD45RA+) cells (Sallusto et al., 2004). The TCM/TM phenotype was dominant amongst HIVRNA+/Gag+ cells (median[range]=40.90%[31.5–60], normalized mean=53.4%), in keeping with observations made for HIV DNA content in ART-treated patients (Figures 3I, S5CD, S6G). Compared to the HIVneg/neg population, HIV-infected cells contained few Tnaive or TTD CD4 and were enriched in both TCM/TM and TEM. Thus, HIV-infected cells do not appear to shift towards a more differentiated phenotype in UNT individuals, in spite of high activation.
Germinal center Tfh are critical for B cell help. Studies using viral outgrowth assays (VOA; (Finzi et al., 1997)) and/or PCR quantitation have shown that Tfh serve as preferential sites of viral replication in lymph nodes in the absence of therapy (Perreau et al., 2013), and may represent a viral reservoir in controlled viremia (Banga et al., 2016). A peripheral blood equivalent of Tfh (pTfh) corresponding to a memory population has recently been identified (Morita et al., 2011) and predicts development of broadly neutralizing antibodies against HIV (Locci et al., 2013). We thus sought to define whether pTfh are preferentially infected. Indeed, pTfh, defined as CD45RA− memory CD4 T cells co-expressing PD-1 and CXCR5, were enriched in HIVRNA+/Gag+ cells (Figures 4AB). Expression of ICOS, a critical co-stimulator for Tfh function, was also highly enriched in HIVRNA+/Gag+, suggesting recent activation (Figure 4C). However, there was no significant difference in expression of CXCR3, a classical Th1 marker whose co-expression identifies a less functional subset of Tfh but can also be induced by activation (Figure S5E). Thus, preferential replication of HIV in activated Tfh cells is not restricted to germinal centers but can also be detected in the periphery.
Blockade of inhibitory co-receptors of TCR signaling is considered a potential means of viral reactivation in “shock and kill” strategies (Deeks, 2012). Besides mediating CD4 T cell exhaustion (Kaufmann et al., 2007), molecules such as PD-1 may contribute to the maintenance of the quiescent state of viral latency in HIV-infected CD4 T cells; the PD-1+ subset is a preferential viral reservoir in ART-treated subjects (Chomont et al., 2009). Expression of multiple inhibitory receptors on CD4 T cells prior to ART was shown to be a predictive biomarker of viral rebound post treatment interruption, suggesting that they may identify those latently infected cells with a higher proclivity to viral transcription (Hurst et al., 2015). However, this link between inhibitory co-receptor expression and spontaneous production of viral mRNA and protein has not been demonstrated in untreated infection. We therefore determined the expression patterns of the receptors PD-1, CTLA-4 and TIGIT on HIV-infected cells, molecules that are all either already targeted by cancer immunotherapies in clinical care or the subject of active drug development (Figures 4D–F, Figures S5F-H). Analysis of individual receptors showed that the PD-1+, TIGIT+ and CTLA-4+ populations were all enriched for HIVRNA+/Gag+ T cells. Indeed, the majority (median=70%) of HIVRNA+/Gag+ CD4 T cells expressed at least one inhibitory receptor, while even in UNT patients a minority of the uninfected, HIVneg/neg CD4 T cells (median=35%) expressed such exhaustion markers (Figures 4GH). The majority of HIVRNA+/Gag+ CD4 T cells expressed PD-1 (median = 63%), in agreement with observations made on HIV DNA content in ART-treated patients, whereas a somewhat smaller fraction expressed TIGIT (median=42%). By analyzing patterns of inhibitory receptor coexpression, we observed that half of the PD-1+ cells also expressed TIGIT, while TIGIT+ only cells were less frequent. The same trends were observed for HIVneg/neg CD4. While the frequency of CTLA-4+ T cells was the lowest for the coreceptors studied, the relative enrichment of HIVRNA+/Gag+ T cells compared to uninfected T cells was greatest for these populations. In particular, while PD-1+ CTLA-4+ and the triple positive (CTLA-4+ PD-1+ TIGIT+) populations represented small subsets (<1%) in the uninfected T cell population, both of these populations were detectable at higher frequencies (~4%) in the HIVRNA+/Gag+ infected T cells. These data show that robust viral replication occurs in blood lymphocytes in spite of high levels of inhibitory receptor co-expression.
Strategies to reduce the latent reservoirs are now being tested in clinical trials (Archin et al., 2012). There is an urgent need for high-throughput assays able to reliably quantify these cells in subjects, but their low frequency makes this challenging. Furthermore, estimation of reservoir size varies widely depending on the assay used (Eriksson et al., 2013), with the VOA giving a minimal value for the replication-competent reservoir and DNA PCR-based assays overestimating its size due to defective viral genomes. Here, we examined ART-treated subjects (Tx, characteristics and cells analyzed, Table S3) to assess the ability of the HIVRNA/Gag assay to quantify latently infected CD4 T cells harboring inducible virus capable of translating Gag and compared it to alternative measurements of reservoir size. As previously, we define this population as the viral translation-competent latent reservoir. In the absence of stimulation, HIVRNA+/Gag+ events were very rare or absent (median[range]=0.55[0–2.6], Figures 5AB), in keeping with published data utilizing HIV Gag protein staining alone, where rare HIVGag+ cells were detected in ART-treated patients (Graf et al., 2013). In contrast, PMA/iono stimulation induced HIVRNA+/Gag+ cells in all but one Tx subject, with frequencies ranging from 1.2 to 660/million (median=3.56, Figures 5AB, Figure S6C). Reactivation of the translation-competent latent reservoir measured by our assay showed a strong trend (p=0.061) towards inverse correlation with CD4/CD8 ratio (Figure 5C) and a weaker inverse correlation with CD4 T cell count (Figure S6A). We next compared the frequency of HIVRNA+/Gag+ events to the estimated size of the reservoir based on integrated or total HIV DNA (Figure 5D). While the size of the reservoir determined by these assays correlated well (Figure 5E, Figure S6B), the median reservoir size as measured by integrated DNA was ~800 copies/million compared to 3.56 cells/million by the HIVRNA/Gag assay. The median ratio between these two measures was 204, which is comparable to the differences detected between integrated DNA and the VOA (Bruner et al., 2015). Factors that may contribute to these differences include the inability of standard DNA assays to distinguish between replication-competent and defective integrated viral genomes (while the HIVRNA/Gag assay detects only cells infected with virus capable of producing viral RNA and protein, thus narrowing estimates of the functional reservoir) and the possibility of multiple integration events in a cell. In addition, the stimulus used may play a role, as not all competent virus may be reactivated by a single round of potent stimulation (Ho et al., 2013) and detection of reactivated virus is limited to those proviruses able to produce Gag protein within the time frame of the assay.
We then compared the HIVRNA/Gag assay to the VOA in a subset of 11 patients (Figure S6DE, Table S4). The HIVRNA/Gag assay and VOA detected a median[range] of 4.65[0–110.4] HIVRNA+/Gag+ translation-competent and 1.43[0.06–32.23] replication-competent HIV-infected cells/million CD4 respectively. In comparison, the median int.DNA copies/million CD4 for these patients was 648. Thus, while the relative frequencies measured by the VOA and HIVRNA/Gag assay varied and did not correlate in this group of patients, they were much closer in magnitude than the PCR-based measure.
We next tested the ability of the protein kinase C modulators bryostatin, an antineoplastic drug currently in clinical cancer trials, and ingenol, currently approved to topically treat actinic keratosis, to induce production of viral mRNA and proteins. Bryostatin, ingenol and their analogues have potent HIV LRA activity in vitro (DeChristopher et al., 2012; Jiang et al., 2014). We detected HIV reactivation in all Tx and UNT subjects examined although at varying degrees (Figure 6ABC). In the majority of Tx patients, induction of the reservoir by both LRAs bryostatin (median[range]=1.2[0.91–37.9]) and ingenol (median[range]=1.38[1.01–3.36]) was lower than that of PMA/iono (median[range]=7.5[0.86–660]). However response to all stimuli varied considerably between donors. In contrast, in UNT subjects the response to bryostatin was close (68–79%) to that of PMA/iono, likely reflecting the major difference in regulation of HIV gene expression in these two contexts. Finally, we examined the phenotype of latently infected cells reactivated with bryostatin and ingenol, as surface markers are much better preserved with these LRAs than with PMA/iono treatment.
In UNT patients, HIV-infected CD4 were predominantly TCM/TTM and TEM in both ongoing and bryostatin-reactivated infection (Figure 6DE). Concordantly, integrated HIV DNA was localized to these compartments (Figure S6F). Though the number of HIVRNA+/Gag+ CD4 more than doubled (Figure 6C) following bryostatin reactivation, the proportion of HIV-infected TCM/TTM compared to TEM was not significantly changed (Figure 6E). This suggests that, in individuals with ongoing viremia, bryostatin is able to reactivate a viral translation-competent reservoir from both the TCM/TM and TEM compartments.
In comparison, in Tx subjects, the majority of bryostatin-reactivated HIVRNA+/Gag+ cells were TEM (Figures 6FG), with TCM contributing a minority fraction to the reactivated population. Indeed, over 90% of bryostatin-reactivated HIVRNA+Gag+ cells were detected in the TEM. In contrast, in a subset of the same patients, ingenol reactivated HIVRNA+/Gag+ cells from both TCM/TTM and TEM in proportions comparable to those in the HIVneg/neg population (Figure 6HI). Interestingly, when the frequency of cells harboring integrated HIV DNA was assessed, both TCM/TTM and TEM contributed to the persistent reservoir (Figures S6GH). Therefore, despite the presence of integrated DNA in both memory subsets, bryostatin-induced reactivation as measured with the HIVRNA/Gag assay was mostly limited to the TEM compartment, while ingenol-induced reactivation was not. This suggests that the differentiation status of CD4 T cells may not affect all LRAs equally, even those from the same class.
Here, we establish and validate a flow-based RNA FISH assay to assess ongoing viral replication and the size of the inducible latent reservoir in HIV-infected individuals, and additionally demonstrate its ability to determine the efficacy of LRAs and the phenotype of the induced latently infected cells. The accurate detection of cells harboring virus able to produce HIV RNA and protein down to frequencies of 0.5–1/million CD4 T cells, combined with the power of single-cell analysis by polychromatic flow cytometry, enabled quantitative and phenotypic characterization of HIV-infected cells directly sampled from patient blood. While previous reports have utilized FISH-based techniques to identify HIV-infected cells (Patterson et al., 2001), the use of concurrent protein staining to identify the translation-competent reservoir allows increased specificity. Our data pinpoint markers of CD4 T cells supporting HIV replication in progressive disease, including features that cannot easily be inferred from in vitro infection, such as enrichment in the pTfh compartment and in the HLA-DR+ subset. Consistent with published data using integrated DNA as a measure of infection (Brenchley et al., 2004) we observe the localization of HIV-infected CD4 in the memory compartment, with limited infection of naïve CD4. We also show that HIV-infected cells are more likely to express markers of exhaustion (PD-1, CTLA-4 and TIGIT) than uninfected CD4 in the context of ongoing viremia. The role for exhaustion markers in the context of CD4 infection remains to be determined – for example, are cells expressing such markers more likely to be infected in vivo, or is expression a consequence of infection itself. As multiple exhaustion markers (including PD-1) are also upregulated as negative feedback mechanisms following activation, an increased susceptibility of these cells to infection is in line with the observations made here and previously (Stevenson et al., 1990) that activated cells are more amenable to HIV infection. In the context of latency, it has been suggested that the expression of multiple inhibitory receptors may identify those CD4 with a higher proclivity to viral transcription (Hurst et al., 2015). The work presented here focuses on CD4 T cells as the major source of infectious virus during chronic infection and the major reservoir in patients receiving therapy. However additional cell types have been reported as permissive to HIV in vivo, including macrophages and dendritic cells. Previous work has demonstrated that monocytes can be assessed (Porichis et al., 2014), thus these subsets could be evaluated by applying the HIVRNA/Gag technique to tissues.
We also narrow down estimates for the size of the inducible reservoir (median 3.56 cell/million CD4 following 12 hr PMA/ionomycin activation, median 204-fold lower than integrated DNA) while demonstrating wide differences amongst subjects with suppressed viral load on therapy. When compared with alternative measurements of reservoir size, the HIVRNA/Gag assay most closely mirrors findings using the VOA, where the minimum size of the replication-competent reservoir is estimated to be 1 per million resting CD4 (1.4 in our cohort), 100–1000 fold less than that measured by integrated DNA. In addition, both the reservoir size as measured by the HIVRNA/Gag assay here and the VOA, shown previously (Kiselinova et al., 2016), correlate with the reservoir measured by integrated HIV DNA. The advantage of the HIVRNA/Gag assay is the direct detection of HIV-infected cells, allowing phenotyping, which is not possible with the VOA. Both assays have the limitation that they may not detect all intact proviruses, due to the stochastic nature of reactivation and the stimuli used. Furthermore, while the VOA detects replication-competent virus (defined by the ability of secreted virus to establish a spreading infection in vitro), the HIVRNA/Gag assay detects cells containing virus able to produce HIV RNA and Gag protein (viral translation-competent virus). Therefore one potential caveat for the HIVRNA/Gag assay is that not all of the reactivated virus is infectious and so the size of the replication-competent reservoir may be slightly overestimated. In contrast, the VOA may underestimate the size of the replication-competent reservoir as virus may be released, but may not establish an in vitro infection and remain undetectable. These differences may explain the lack of correlation observed between these two assays and the larger reservoir size detected using the HIVRNA/Gag assay when compared to the VOA.
An additional factor in the detection of rare cells is the probability of detecting events due to Poisson distribution and sampling differences. To increase the probability of accurately detecting rare cells, increasing cell numbers must be analyzed. In the current study, 2–3 million CD4 T cells per patient per condition were usually acquired on the flow cytometer. The requirement for high cell numbers may be a limiting factor for latency studies; however, a similar restriction exists for known techniques to measure latent reservoirs.
Finally, we show that this approach can be used to assess the efficiency of LRAs such as bryostatin and ingenol, drugs currently in clinical trials, and importantly determine the susceptibility of distinct CD4 cells to LRA-induced reactivation. The need for such primary cell assays is highlighted by the wide variability of results obtained in in vitro latency models (Spina et al., 2013). The phenotypic analysis of LRA-induced cells has important potential implications for the function of LRAs. Firstly, while both the TEM and TCM CD4 pools contain integrated pro-virus, the relative frequencies of functional versus defective pro-viral DNA have been suggested to differ between subsets (Soriano-Sarabia et al., 2014). Alternatively, CD4 subsets may vary in their sensitivity to individual LRAs. While these two mechanisms are not mutually exclusive, our data suggest a differential sensitivity of CD4 populations to individual LRAs: bryostatin readily induced the TEM reservoir, but had limited effect on the TCM compartment, contrasting with the more even effect observed with ingenol. An effective LRA must induce HIV protein expression in all latently infected cells regardless of phenotype to enable recognition and elimination by host immune responses, and as such ingenol may represent a promising candidate. Combinations of LRAs need to be assessed, to increase potency but also to recruit additional subsets of latently infected cells that may not be amenable to reactivation with a single drug. This technology and the results obtained may have important implications for HIV pathogenesis studies, including investigation of early transmission events, testing of LRAs and monitoring of cure strategies.
Leukaphereses were obtained from study participants at the Montreal General Hospital, Montreal, Canada and at Martin Memorial Health Systems, Florida, USA. The study was approved by the respective IRBs and written informed consent obtained from all participants prior to enrolment. See Supplemental Experimental Procedures for details. Untreated, viremic participants (UNT) were either treatment naïve, or untreated for at least 6 months. Treated subjects (Tx) were on ART for over 12 months with controlled viral load (<50 vRNA copies/mL) for at least 6 months. Patient characteristics are summarized in Tables S2–S4. In rare cases, due to limited sample availability, sequential leukaphereses were used for individual subjects. PBMC isolated by Ficoll density gradient were stored in liquid nitrogen.
CD4 T cells were isolated from PBMC by negative magnetic bead selection (StemCell), resulting in an untouched population defined as CD3+CD4+/-CD8-CD14-CD19- (purity routinely over 95%). Cells were stimulated for 36–40 hr in RPMI with PHA-L (10μg/ml, Sigma) and IL-2 (50U/ml), then washed and maintained for 6–7 days in RPMI with IL-2 (100U/ml). In some experiments, ARVs (T20 (7.5μg/ml) + AZT (1μM)) were added. Enfuvirtide (T-20), Zidovudine (AZT), and IL-2 (Lahm and Stein, 1985) were obtained through NIH AIDS Reagent Program, Division of AIDS, NIAID, NIH: human rIL-2 from Dr. Maurice Gately, Hoffmann - La Roche Inc.
CD4 T cells were isolated as above, resuspended at 2 × 106/ml media with ARVs (T20 + AZT, as before) and rested for 3–5 hr. Cells were either unstimulated, stimulated for 12 hr with PMA (50ng/ml) and ionomycin (0.5μg/ml), or for 18 hr with Bryostatin-1 (10nM, Enzo Life Sciences) or Ingenol-3-angelate (25nM, Sigma). 5–12 × 106 purified CD4 were required per patient/condition.
See Figure S1 for the workflow schematic. Samples were subjected to the PrimeFlow RNA assay (Affymetrix/eBioscience) as per manufacturer’s instructions. See Supplemental Experimental Procedures for protocol details and antibody panels. Cells were stained for viability, surface stained for phenotypic markers and stained intracellulary for HIV Gag protein prior to mRNA detection. Samples were acquired on an LSRII (BD Bioscience). Analysis was performed using FlowJo (Treestar, V10).
Reactivated, HIV-replicating CD4 T cells from an untreated patient were spiked into uninfected cells at different ratios to set up a dilution series. The predicted frequency of HIVRNA+/Gag+ (or HIVRNA+ or HIVGag+) was compared to the detected frequency. See Supplemental Experimental Procedures for details.
Patient reactivated CD4 T cells were sorted according to expression of Gag protein and GagPol mRNA. The number of nuclear and total gag-pol mRNA spots and CTCF was determined by confocal microscopy. See Supplemental Experimental Procedures for details.
Quantifications of total and integrated HIV DNA were determined as previously described (Vandergeeten et al., 2014).
Quantifications of replication-competent virus were performed as previously described (Siliciano and Siliciano, 2005).
All statistical analyses were performed in Prism (V6, GraphPad). Data was tested for normality using the D’Augustino-Pearson Omnibus normality test. Where appropriate, parametric tests were applied. Statistical tests were two-sided and repeated measures used for comparisons within subjects. For comparisons between groups, Kruskal-Wallis or Friedman one-way ANOVA with Dunn’s post-test was used. For correlations, Spearman’s R (Rs) correlation coefficient was used. For pair-wise analysis of non-normally distributed data, Wilcoxon Signed Rank t-tests were used. P<0.05 were considered significant.
We thank Josée Girouard, the clinical staff at McGill University Health Centre and all study participants; Drs Dominique Gauchat and the CRCHUM Flow Cytometry Platform, Daniel Zenklusen and Chunfai Lai for technical assistance; Dylan Malayter for reagents and Drs Shane Crotty and Naglaa Shoukry for their input on this manuscript.
This study was supported by the National Institutes of Health (HL-092565, AI100663 CHAVI-ID, AI113096, AI118544 and the Delaney AIDS Research Enterprise (DARE) 1U19AI096109); the Canadian Institutes for Health Research (grant #137694; Canadian HIV Cure Enterprise), a Canada Foundation for Innovation grant, the FRQS AIDS and Infectious Diseases Network and the Foundation for AIDS Research (108928-56-RGRL). D.E.K and N.C. are supported by FRQS Research Scholar Awards. A.F. is the recipient of a Canada Research Chair. J.P.R is the holder of Louis Lowenstein Chair, McGill University. J.R. is the recipient of a CIHR Fellowship Award #135349. N.A. is the recipient of a King Abdullah scholarship from the Saudi Government.
AUTHOR CONTRIBUTIONSA.E.B, J.N., F.P, A.F., N.C. and D.E.K. designed the studies; A.E.B., J.N., R.F., J.R., R.C., N.B., G.G.D., M.M, and N.A. performed experiments; J.P.R. obtained IRB approval and recruited participants; B.D.W. provided input on study design; A.E.B. and D.E.K. interpreted the data and wrote the paper with all co-authors’ assistance.
The authors have no conflicts of interest to report.
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