JAIDS Journal of Acquired Immune Deficiency Syndromes:
Basic and Translational Science
HIV-1 Is Not a Major Driver of Increased Plasma IL-6 Levels in Chronic HIV-1 Disease
Shive, Carey L. BA*,†; Biancotto, Angélique PhD‡; Funderburg, Nicholas T. PhD*,†; Pilch-Cooper, Heather A. BS*,†; Valdez, Hernan MD§; Margolis, Leonid PhD‡; Sieg, Scott F. PhD*,†; McComsey, Grace A. MD‖,†; Rodriguez, Benigno MD, MSc, FIDSA*,†; Lederman, Michael M. MD*,†
*Division of Infectious Diseases, Case Western Reserve University School of Medicine, Cleveland, OH
†University Hospitals, Case Medical Center, Cleveland, OH
‡Laboratory of Molecular and Cellular Biophysics, National Institute of Child Health and Human Development, Bethesda, MD
§Pfizer Inc, New York, NY
‖Department of Pediatrics, Center for AIDS Research, Case Western Reserve University School of Medicine, Cleveland, OH.
Correspondence to: Michael M. Lederman, MD, Case Western Reserve University School of Medicine, 2061 Cornell Rd, Cleveland, OH 44106 (e-mail: email@example.com).
Supported by the Center for AIDS Research at Case Western Reserve University, AI-36219, and by the Tissue Procurement, Histology, and Immunohistochemistry Core Facility of the Case Comprehensive Cancer Center CA43703 and by grant awards from the Fasenmyer Foundation and AI-76174 from the National institute of Health.
Dr M.M.L has received grant support and has consulted for Pfizer. Dr H.V. is employed by Pfizer. G.A.M has served as a scientific advisor for Bristol Myers Squibb, GlaxoSmithKline, Abbott, Tibotec, and Gilead Sciences; has received research grants from Bristol Myers Squibb, GlaxoSmithKline, Abbott, Merck, and Gilead Sciences; and is currently serving as the DSMB Chair for a Pfizer-sponsored study.
All other authors have no conflicts of interest to disclose.
The authors C.S., A.B., N.F., and H.C. performed experiments. H.V. provided patient samples. B.R. provided statistical method support. All authors contributed to the analysis of data and writing of the article.
Supplemental digital content is available for this article. Direct URL citations appear in the printed text and are provided in the HTML and PDF versions of this article on the journal's Web site (www.jaids.com).
Received February 6, 2012
Accepted May 4, 2012
Objective: Increased plasma IL-6 levels have been associated with HIV-1 disease progression risk, yet the drivers of IL-6 production in HIV-1 infection are not known. This study was designed to explore the relationship between HIV-1 replication and IL-6 induction.
Design: Correlations between plasma levels of IL-6 and HIV-1 RNA were examined in 2 clinical studies. To more directly assess the induction of IL-6 by HIV-1, several cell and tissue types that support HIV-1 replication in vivo were infected with HIV-1, and expression of IL-6 was measured.
Methods: Spearman rank correlations were used to examine the relationship between plasma levels of IL-6 and HIV-1 RNA. Macrophages and colonic and lymph node histocultures were infected with HIV-1 or stimulated with bacterial products, lipopolysaccharide (LPS) or flagellin, and IL-6 levels in supernatant were measured by enzyme-linked immunosorbent assay or multiplex bead assay.
Results: In the clinical studies, there was weak or no correlation between plasma levels of IL-6 and HIV-1 RNA, but IL-6 levels were correlated with plasma levels of the LPS coreceptor CD14. Macrophages stimulated with LPS or flagellin showed robust production of IL-6, but there was no increase in IL-6 production after HIV-1 infection. IL-6 expression was not increased in lymph node histocultures obtained from HIV-1–infected subjects nor after productive HIV-1 infection of colonic or lymph node histocultures ex vivo.
Conclusions: We find no evidence that HIV-1 replication is an important driver of IL-6 expression in vivo or in in vitro systems.
Chronic immune activation is a major predictor of HIV-1 disease progression. Increased expression of CD38 and HLA-DR on T cells is an indicator of this immune activation1–3 as are plasma levels of cytokines such as IL-6 and TNFa.4 The advent of highly active antiretroviral therapy has greatly extended the life expectancy of persons infected with HIV-1, however, even with controlled viral replication, HIV-1–infected patients are at increased risks for morbidities including cancer, liver disease, and cardiovascular disease.5 Though viral replication has been linked to many of these indices of immune activation, many remain elevated even when viral replication is “fully” suppressed by highly active antiretroviral therapy.1,6,7 In the SMART trial of sustained versus intermittent antiretroviral therapy, 3 soluble factors were independent predictors of overall and cardiovascular morbidities as follows: IL-6, C-reactive protein, and D-dimers.8 In a nested case–control substudy of the SMART trial, plasma levels of soluble CD14 (sCD14) a coreceptor for bacterial lipopolysaccharide (LPS) were also an independent predictor of mortality.9 In other studies, increased plasma IL-6 levels have been associated with new AIDS-defining illnesses or death,10 the progression of clinical disease,11–13 and the development of opportunistic infections.14 Although it is clear that increased plasma IL-6 is associated with HIV-1 disease progression; it remains unclear what is driving the increased levels of IL-6 in HIV-1 disease. This study was designed to explore the relationship between HIV-1 replication and increased plasma levels of IL-6 in persons with HIV-1 infection. We found little indication that HIV-1 replication plays an important role in the elevated levels of IL-6 found in the plasma of HIV-1–infected subjects, as plasma levels of IL-6 correlated weakly or not at all with plasma levels of HIV-1 RNA, and we could not find increased levels of IL-6 in supernatants of macrophages, lymph nodes, or colonic histocultures after in vitro infection with HIV-1.
These studies were approved by the institutional review board at University Hospitals/Case Medical Center and for the Maraviroc versus Efavirenz in Treatment-Naive Patients (MERIT) study by the Institutional Review Boards or Independent Ethics Committees of all participating sites. All patients provided written informed consent in accordance with the Declaration of Helsinki.
The MERIT Study compared the effects of maraviroc or efavirenz added to a treatment regimen containing zidouvudine and lamivudine among treatment-naive HIV-1–infected persons.15 Stored samples obtained from 60 trial participants (30 receiving Maraviroc (MVC) and 30 treated with efavirenz) who controlled viremia on these regimens were analyzed for markers of immune activation (CD38) and for markers of inflammation and coagulation (IL-6, D-dimers, TNFrI, TNFrII, and hs C-reactive protein) in plasma and comparisons between the study arms have been reported earlier.16 In these subjects, median HIV-1 RNA level was 4.9 log10 copies per milliliter and the median CD4 T-cell count was 274 cells per microliter (see Table, Supplemental Digital Content 1, http://links.lww.com/QAI/A335). The second clinical study was a cross-sectional study of 154 HIV-1–infected patients who were receiving care at University Hospitals/Case Medical Center. The median CD4 T-cell count was 350 cells per microliter, and the HIV-1 RNA level in plasma ranged from <50 copies per milliliter to >750,000 copies per milliliter. Stored plasma samples also were analyzed for levels of IL-6 and sCD14.
Whole pelvic lymph nodes were obtained from 11 HIV-1–infected adults and 10 uninfected adults who were undergoing medically indicated surgery at University Hospitals of Cleveland (Cleveland, OH). Lymphocyte phenotypes and spontaneous expression of cytokines were reported earlier.17
Normal human colonic mucosal tissue was obtained through the Tissue Procurement, Histology, and Immunohistochemistry Core Facility of the Case Comprehensive Cancer Center. Colonic tissue was cleaned of muscle and fat, and then mucosa was cut into 3-mm × 3-mm explants for histoculture as described previously.18,19
Virus Preparation and Storage
HIV-1Ba-L was propagated in a PM1 cell line (kindly provided by Dr Donald E. Mosier, Scripps Research Institute, La Jolla, CA), which is permissive for growth of macrophage and T-cell tropic HIV-1 viruses. PM1 cells were grown in Roswell Park Memorial Institute (RPMI) RPMI 1640 (BioWhittaker Lonza, Walkersville, MD) containing 10% Fetal Bovine Serum (Gemini Bio-Products, West Sacramento, CA), 2 mM L-Glutamine (Biowhittaker Lonza), and 100 Units/mL Penicillin/Streptomycin (BioWhittaker Lonza). Supernatants from uninfected PM1 cells were used as controls for infection experiments. Undiluted HIV-1Ba-L viral stock propagated in PM1 cells contained <0.5 pg/mL IL-6.
HIV-1 Infection of Macrophages
Monocytes were obtained from heparinized whole blood of healthy, HIV-1–uninfected subjects by mixing whole blood with RosetteSep monocyte enrichment antibody cocktail (StemCell Technologies, Vancouver, British Columbia, Canada) and incubating for 20 minutes at room temperature following manufacturer's instructions. Blood was then separated over Ficoll; unbound monocytes separated at the Ficoll-plasma interface and unwanted cell types pelleted with the erythrocytes. Enriched monocytes were plated in complete medium consisting of RPMI (Lonza, Walkersville, MD), 10% Fetal Bovine serum (Gemini Bio-Products), 1% L-glutamine, and 1% penicillin streptomycin (Lonza, Walkersville, MD) at 1 million cells per milliliter in 24-well Falcon tissue culture plates (Becton Dickinson and Company, Franklin Lakes, NJ) for 7 days, with medium replacement on day 4. On day 7, supernatant was collected and frozen. Macrophages were then infected overnight with HIV-1Ba-L at 100, 1000, or 10,000 TCID50 or stimulated with 50 ng/mL LPS (Sigma-Aldrich, St Louis, MO) or with 1 ug/mL flagellin (Invivogen, San Diego, CA). After overnight infection or stimulation, supernatant was collected and fresh complete medium was added to all wells. The wells stimulated with LPS or flagellin received new medium containing fresh LPS or flagellin. Supernatants were collected at days 1, 3, 7, 10, and 14 after infection or stimulation.
IL-6 levels in supernatant from colonic and macrophage cultures were measured using a human IL-6 enzyme-linked immunosorbent assay (ELISA) kit (Quantikine) or a high sensitivity IL-6 ELISA kit (Quantikine HS) both from R&D Systems (Minneapolis, MN). Supernatants harvested from lymph node histocultures were tested for IL-6 levels using a multiplex bead array assay as described previously.17
Colonic Mucosal Histoculture
Two 3-mm × 3-mm colonic explants were placed in 100 uL of RPMI 1640 (BioWhittaker Lonza) supplemented with 15% Fetal Bovine Serum (Gemini Bio-Products), 0.1 mM MEM-nonessential amino acids (Gibco Invitrogen, Grand Island, NY), 2.5 μg/mL Fungizone (Gibco Invitrogen), 1 mM Minimum Essential Medium MEM-Sodium Pyruvate (Gibco Invitrogen), 100 units/mL Penicillin/Streptomycin (BioWhittaker Lonza), and 50 μg/mL Gentamicin (Gibco Invitrogen) in a 96-well flat-bottomed plate and incubated for 1 hour at 37°C in 5% CO2 to equilibrate before infection. After 1 hour, 1 × 104 TCID50 HIV-1Ba-L in 100 μL or 100 μL of control supernatant from the uninfected PM1 cell line was added to each well. Explants were incubated with virus or control supernatant for 2 hours at 37°C in 5% CO2, then washed with phosphate-buffered saline. After the wash step, tissues were placed on Gelfoam absorbable gelatin sponges (Pfizer, New York, NY) that had been soaked in medium in 24-well plates for 1 hour at 37°C in 5% CO2. Plates containing explants on Gelfoam at the air–liquid interface20 were incubated at 37°C in 5% CO2. Supernatants were collected at the indicated times and frozen at −80°C for later analysis.
HIV-1 P24 Measurement
P24 ELISA assay plates/kits were kindly provided by Dr John Sullivan and Dr Katherine Luzuriaga, (University of Massachusetts Medical Center) and were used for measurement of HIV-1 p24 levels in supernatant as described previously.21
Lymph Node Histoculture
Lymph nodes were dissected, and tissue blocks were placed on collagen sponge gels and cultured at the air–liquid interface for 15 days as described previously.17,20 Using HIV-1 p24 ELISA, we detected HIV-1 replication in tissues of 8 of 11 patients with HIV-1, with average levels of 1046 pg/mL (range: 645–2462 pg/mL).17 Ten lymph node sections prepared from the nodes of healthy controls were infected overnight with approximately 300 TCID50 of HIV-1 LAI.04virus per block. Sections were then washed with phosphate-buffered saline and cultured in fresh medium, and medium was changed every 3 days thereafter. Supernatant was pooled from each subject's samples and was tested for IL-6 levels as noted above.
Plasma levels of IL-6, HIV-1 RNA, and other biomarker levels were compared using Spearman rank correlation method. Differences between groups were compared using Mann–Whitney U tests.
Plasma IL-6 Levels Correlate Weakly With Plasma HIV-1 RNA Levels Before Administration of Antiretroviral Therapies
In the MERIT study at baseline, before initiation of antiretroviral therapy, plasma IL-6 levels were correlated to plasma HIV-1 RNA levels (r = 0.2949; P = 0.0261, Fig. 1A). By weeks 4 and 12 after the initiation of therapy, plasma levels of HIV-1 and IL-6 were no longer significantly correlated (Figs. 1B, C). IL-6 levels remained elevated when compared with levels seen in uninfected controls6 and did not decrease significantly until week 48 (Mann–Whitney P = 0.0112) irrespective of the dramatic and early decreases in plasma HIV-1 RNA levels (Fig. 1D).
Next, we analyzed data from a cross sectional study performed among 154 HIV-1–infected patients who were receiving care at University Hospitals/Case Medical Center. Plasma levels of IL-6 and sCD14 and HIV-1 RNA were measured. In this patient cohort, the median CD4 T-cell count was 350 cells per microliter, and plasma HIV-1 RNA levels ranged from <50 copies per milliliter to >750,000 copies per milliliter. There was no correlation between plasma levels of IL-6 and plasma levels of HIV-1 RNA (Fig. 2A). On the other hand, soluble CD14 levels in plasma correlated significantly with both plasma HIV-1 RNA levels (Fig. 2B; r = 0.4216; P < 0.0001) and with IL-6 levels (Fig. 2C; r = 0.3016; P = 0.0009). Considering the weak relationship between IL-6 levels and HIV-1 RNA levels in plasma in these clinical studies, we next asked if we could demonstrate the induction of IL-6 expression in primary cells and in histocultures by HIV-1 exposure and replication.
HIV-1 Infection of Monocyte-Derived Macrophages Does Not Induce IL-6 Production
Monocytes were negatively selected from whole blood obtained from 2 HIV-1–uninfected subjects. Enriched monocytes were placed in plastic 24-well tissue culture plates in complete medium and allowed to mature for 7 days. After maturation, replicate wells containing monocyte-derived macrophages were incubated overnight with medium alone or with LPS (50 ng/mL), flagellin (1 ug/mL), or with HIV-1 Ba-L 1000 and 10,000 TCID50. LPS or flagellin exposure induced substantial expression of IL-6 that ranged from 11.5 to 2288 pg/mL at day 3 (Table 1). In triplicate wells, macrophages became actively infected as reflected by increasing HIV-1 p24 levels in supernatants (Table 1). Despite productive HIV-1 infection, levels of IL-6 were not increased in the culture supernatants at any time in these infected wells from day 3 to day 14. In a third similar experiment (not shown), exposure of monocyte-derived macrophages to HIV-1Ba-L did not result in productive HIV-1 infection in any well. In these wells too, IL-6 levels were not increased above levels in unexposed wells (not shown). This indicates that neither productive HIV-1 replication nor exposure to HIV-1 virions without infection could induce IL-6 expression. Unstimulated peripheral blood mononuclear cells (PBMCs) isolated from whole blood were also incubated overnight with medium, LPS (50 ng/mL), flagellin (1 μg/mL), or with HIV-1Ba-L. As was seen among monocyte-derived macrophages, no IL-6 was induced by HIV-1 infection of PBMC, yet exposure to LPS or flagellin induced substantial levels of IL-6 (data not shown).
HIV-1 Infection of Colonic Histocultures Does Not Induce IL-6 Production
Because mucosal and secondary lymphoid tissues are the major sites of HIV-1 replication in vivo, we asked if HIV-1 infection of these tissues could induce production of IL-6. Colonic biopsies from 3 HIV-1–uninfected subjects (C3, C4, C5) were infected ex vivo with HIV-1Ba-L for 2 hours then washed. Sections were cultured on absorbable gelatin sponges for 2 weeks at the air–liquid interface.20 Culture medium was collected and replaced with new medium on days 1, 3, 7, 10, and 14. Viral infection was confirmed by documenting increases in HIV-1 p24 levels in supernatant by ELISA (data not shown) and IL-6 levels were measured by ELISA. Although productive infection and IL-6 production were documented in the virus-exposed histocultures, no difference was noted between the levels of IL-6 generated by the infected histocultures when compared with the levels generated by the uninfected tissues at any time point (Fig. 3).
Lymph Node Histocultures Infected With HIV-1 In Vivo or Ex Vivo Do Not Increase IL-6 Production
Lymph node samples obtained by surgical biopsy from 11 HIV-1+ patients and 10 uninfected subjects were cut into sections and cultured on collagen sponge gels at the air–liquid interface. Sections from the 10 uninfected subjects were cultured in medium or infected overnight with HIV-1LAI.04. The following day the sections were washed, and new medium was added. Culture supernatants were collected every 3 days, and IL-6 was measured using a multiplex bead array assay.17 Figure 4 shows the accumulated levels of IL-6 produced by lymph node cultures from 11 HIV-1+ patients (chronic), 10 uninfected subjects (uninfected), and 10 lymph node sections from the same uninfected subjects that were infected by overnight exposure to HIV-1 LAI.04 (acute). There was no difference in IL-6 levels in lymph node samples from controls that were left uninfected (uninfected, median 17,528 pg/mL) or were infected with HIV-1 (acute, median 19,571 pg/mL). Interestingly, levels of IL-6 produced spontaneously by lymph node histocultures from HIV-1–infected patients (chronic; median 2437 pg/mL) were significantly lower than levels produced by the uninfected or ex vivo infected histocultures (Mann–Whitney U test, P = 0.0288 and P = 0.0232, respectively). This may represent a depletion of IL-6–producing cells in the chronically infected node17 or a failure of spontaneous IL-6 expression in the chronically infected tissues.
Although increased plasma levels of IL-6 have been linked to risk of HIV-1 disease progression in some4,8,10,11,13 but not all studies,22 the determinants of IL-6 induction and immune activation in this setting are incompletely understood. Here we report the results of 2 clinical studies in which the relationship between plasma HIV-1 RNA levels and IL-6 are explored. In the first, an antiretroviral therapy trial among treatment-naive subjects (MERIT), pre-treatment HIV-1 RNA levels in plasma correlated weakly with plasma IL-6 levels, but this relationship disappeared rapidly as HIV-1 RNA levels fell with application of antiretroviral therapies. Plasma levels of IL-6 did not decrease significantly until 48 weeks of therapy (Mann–Whitney P = 0.0112) but never reached levels seen in uninfected persons. Thus, the correlation between HIV-1 RNA levels and IL-6 levels in plasma was weak at baseline and disappeared with suppression of HIV-1 replication as the substantial decrease in HIV-1 replication in the first weeks of therapy were not reflected by a decrease in the plasma levels of IL-6. In a different study where plasma cytokines and HIV-1 RNA levels were monitored early after introduction of antiretroviral therapy, although HIV-1 RNA levels fell rapidly and significantly within the first few days of therapy, plasma levels of IL-6 did not decrease durably even after 24 weeks of therapy.23 In another large study that involved more than 1000 HIV-1–infected patients, examining the association of low-level viremia with inflammation and mortality, HIV-1 RNA was only significantly associated with plasma IL-6 levels when virus levels exceeded 10,000 copies per milliliter.24 Interestingly, this association was strongly influenced by the CD4 T-cell count.24
In the second clinical study reported here, a cross-sectional study of a heterogeneous population of HIV-1–infected adults, only a weak but statistically not significant relationship between plasma levels of IL-6 and HIV-1 RNA levels could be demonstrated. In a recently published study, we found that plasma levels of IL-6 remained elevated in patients who had therapy-controlled viremia (<400 copies/mL) for an average of more than 7 years. Importantly, IL-6 levels were significantly higher in subjects who failed to increase their CD4 T-cell counts to levels >350 cells per microliter than in subjects whose CD4 T-cell counts had increased to levels >500 cells per microliter.25 Although other studies have also found a weak relationship between plasma levels of IL-6 and HIV-1 RNA,9,26 the determinants of high level IL-6 expression in HIV-1 infection seem to be complex, and there is dissociation between levels of HIV-1 RNA and levels of IL-6 in the plasma of patients, especially during the dynamic changes in HIV-1 replication after the introduction of antiretroviral therapy.
As the immunologic and inflammatory interactions in HIV-1 infection are complex, we decided to utilize simpler systems of primary cell and histoculture models to ascertain if HIV-1 replication could induce IL-6 expression. Using unstimulated PBMC, macrophages, lymph nodes, and colonic mucosal histocultures, we could not find any evidence that ex vivo HIV-1 exposure or productive infection could drive IL-6 production in any of these systems. Although macrophages did not express IL-6 after HIV-1 exposure and infection, incubation with bacterial products, LPS and flagellin, induced high-level expression of IL-6. We also examined the expression of IL-6 in lymph node histocultures obtained from subjects who were HIV-1–infected and found that the spontaneous expression of IL-6 in these histocultures was actually less than in histocultures prepared from lymph nodes of uninfected controls.
Very high levels of IL-6 were produced by colonic histocultures whether HIV-1–infected or not and relatively high levels of IL-6 also accumulated in lymph node histocultures whether HIV-1 infected or not. The relatively high background levels of IL-6 seen in the colonic mucosal histocultures could be a consequence of exposure to colonic bacteria in vivo, and this might have obscured induction of IL-6 by HIV-1 infection ex vivo. On the other hand, gut mucosal cells could be an important source of systemic IL-6 levels in vivo. Conceivably, greater exposure of mucosal immune cells to microbes and their products as a consequence of the sustained damage to gut mucosal integrity in HIV-1 infection27,28 may underlie the high levels of IL-6 typically found in untreated and treated HIV-1 infection. In this regard, a recent study examining a mouse model of colitis showed that microbiota of the gut could induce the production of IL-6 by dendritic cells, and this could promote T-cell activation and colitis.29 Although we show here a good correlation between plasma levels of IL-6 and the LPS coreceptor sCD14, we did not have samples available for measurement of LPS. We had earlier reported elevated plasma levels of IL-6 in patients with controlled viremia but who experienced incomplete immune restoration.6 On analysis of that data set, we can now report that plasma IL-6 levels were correlated with plasma LPS levels (Spearman rho; r = 0.287, P = 0.009, n = 81).6 Marchetti et al22 found that untreated patients with higher plasma levels of LPS also tended to have higher levels of IL-6 (P = 0.053).
The lack of induction of IL-6 expression in vitro by HIV-1 replication is consistent with earlier reports that in vitro HIV-1 infection of PBMCs or macrophages alone does not induce IL-6 production.30,31 Molina et al30 infected PBMC overnight with HIV-1 and then examined culture supernatant for IL-1b, IL-6, and TNFa. They did not detect induction of any of these cytokines by HIV-1, however, PBMC exposed to LPS at concentrations as low as 0.5 ng/mL expressed significant amounts of IL-1b, IL-6, and TNFa. On the other hand, Nakajima et al32 showed that PBMC exposed to either live or inactivated HIV-1 could produce IL-6 as measured by the IL-6–dependent proliferation of the murine cell line MH60.BSF-2. Gan et al31 infected monocyte-derived macrophages with HIV-1Ba-L and saw no induction of IL-6. When HIV-1–infected cells were also incubated with LPS, levels of IL-6 mRNA were 7-fold higher than in uninfected cells that were exposed to LPS alone. HIV-1 proteins Tat33,34 and Vpr35 have been reported to induce IL-6 gene expression, however, these studies reported only the effects of recombinant viral proteins and not the induction of IL-6 by whole virus infection. We did not explore the effects of HIV-1 exposure on transcription of IL-6 RNA in any of the systems we employed. Thus, it is conceivable that HIV-1 exposure induces IL-6 transcription and cytokine synthesis but that the cytokine is degraded or absorbed by cells within these preparations. Should this be the case in vivo, we still cannot attribute the high systemic levels of IL-6 in HIV-1 infection to HIV-1 replication.
It is worth noting that IL-6 can reactivate provirus expression in HIV-1–infected macrophages,36 so it is possible that the weak correlations seen between plasma levels of IL-6 and HIV-1 RNA may be a consequence of IL-6 induction of latent virus expression rather than the other way around.
In summary, the correlations between HIV-1 RNA and IL-6 levels in plasma were weak at best, and we could find no evidence that HIV-1 infection could induce IL-6 expression in vitro. These findings suggest that HIV-1 replication does not directly drive the high systemic levels of IL-6 found in HIV-1 disease. The correlations we found between IL-6 and other indices of inflammation, such as sCD14, suggest that IL-6 levels are associated with the general immune activation and inflammation that are demonstrable even when HIV-1 replication is well controlled by antiretroviral therapy. What is inducing this continued immune activation and inflammation remains a question. We suspect that this may be related to the apparent persistent defect in gut mucosal integrity seen even in treated HIV-1 infection37 and the local and systemic exposure to gut-derived microbial products that can drive IL-6 expression in vitro and in vivo.
The authors wish special thanks to Linda Lambrecht at University of Massachusetts Medical Center for her assistance with the p24 ELISA plates.
1. Hunt PW, Martin JN, Sinclair E, et al.. T cell activation is associated with lower CD4+ T cell gains in human immunodeficiency virus-infected patients with sustained viral suppression during antiretroviral therapy. J Infect Dis. 2003;187:1534–1543.
2. Giorgi JV, Hultin LE, McKeating JA, et al.. Shorter survival in advanced human immunodeficiency virus type 1 infection is more closely associated with T lymphocyte activation than with plasma virus burden or virus chemokine coreceptor usage. J Infect Dis. 1999;179:859–870.
3. Anthony KB, Yoder C, Metcalf JA, et al.. Incomplete CD4 T cell recovery in HIV-1 infection after 12 months of highly active antiretroviral therapy is associated with ongoing increased CD4 T cell activation and turnover. J Acquir Immune Defic Syndr. 2003;33:125–133.
4. Connolly NC, Riddler SA, Rinaldo CR. Proinflammatory cytokines in HIV disease-a review and rationale for new therapeutic approaches. AIDS Rev. 2005;7:168–180.
5. Smith C, Sabin CA, Lundgren JD, et al.. Factors associated with specific causes of death amongst HIV-positive individuals in the D: A:D Study. AIDS. 2010;24:1537–1548.
6. Lederman MM, Calabrese L, Funderburg NT, et al.. Immunologic failure despite suppressive antiretroviral therapy is related to activation and turnover of memory CD4 cells. J Infect Dis. 2011;204:1217–1226.
7. Marchetti G, Gori A, Casabianca A, et al.. Comparative analysis of T-cell turnover and homeostatic parameters in HIV-infected patients with discordant immune-virological responses to HAART. AIDS. 2006;20:1727–1736.
8. Kuller LH, Tracy R, Belloso W, et al.. Inflammatory and coagulation biomarkers and mortality in patients with HIV infection. PLoS Med. 2008;5:e203.
9. Sandler NG, Wand H, Roque A, et al.. Plasma levels of soluble CD14 independently predict mortality in HIV infection. J Infect Dis. 2011;203:780–790.
10. Kalayjian RC, Machekano RN, Rizk N, et al.. Pretreatment levels of soluble cellular receptors and interleukin-6 are associated with HIV disease progression in subjects treated with highly active antiretroviral therapy. J Infect Dis. 2010;201:1796–1805.
11. Breen EC, Rezai AR, Nakajima K, et al.. Infection with HIV is associated with elevated IL-6 levels and production. J Immunol. 1990;144:480–484.
12. Mildvan D, Spritzler J, Grossberg SE, et al.. Serum neopterin, an immune activation marker, independently predicts disease progression in advanced HIV-1 infection. Clin Infect Dis. 2005;40:853–858.
13. Lafeuillade A, Poizot-Martin I, Quilichini R, et al.. Increased interleukin-6 production is associated with disease progression in HIV infection. AIDS. 1991;5:1139–1140.
14. Rodger AJ, Fox Z, Lundgren JD, et al.. Activation and coagulation biomarkers are independent predictors of the development of opportunistic disease in patients with HIV infection. J Infect Dis. 2009;200:973–983.
15. Cooper DA, Heera J, Goodrich J, et al.. Maraviroc versus efavirenz, both in combination with zidovudine-lamivudine, for the treatment of antiretroviral-naive subjects with CCR5-tropic HIV-1 infection. J Infect Dis. 2010;201:803–813.
16. Funderburg N, Kalinowska M, Eason J, et al.. Effects of maraviroc and efavirenz on markers of immune activation and inflammation and associations with CD4+ cell rises in HIV-infected patients. PLoS One. 2010;5:e13188.
17. Biancotto A, Grivel JC, Iglehart SJ, et al.. Abnormal activation and cytokine spectra in lymph nodes of people chronically infected with HIV-1. Blood. 2007;109:4272–4279.
18. Fletcher PS, Elliott J, Grivel JC, et al.. Ex vivo culture of human colorectal tissue for the evaluation of candidate microbicides. AIDS. 2006;20:1237–1245.
19. Grivel JC, Margolis L. Use of human tissue explants to study human infectious agents. Nat Protoc. 2009;4:256–269.
20. Glushakova S, Baibakov B, Margolis LB, et al.. Infection of human tonsil histocultures: a model for HIV pathogenesis. Nat Med. 1995;1:1320–1322.
21. Hesselton RM, Greiner DL, Mordes JP, et al.. High levels of human peripheral blood mononuclear cell engraftment and enhanced susceptibility to human immunodeficiency virus type 1 infection in NOD/LtSz-scid/scid mice. J Infect Dis. 1995;172:974–982.
22. Marchetti G, Cozzi-Lepri A, Merlini E, et al.. Microbial translocation predicts disease progression of HIV-infected antiretroviral-naive patients with high CD4+ cell count. AIDS. 2011;25:1385–1394.
23. Funderburg N. Delayed Reduction in CD4 T Cell Turnover Following Viral Control Correlates With Markers of Microbial Translocation in Treatment-Naive Patients Receiving RAL-Based ART: Preliminary Results From ACTG A5248. Boston, MA: CROI; 2011:189.
24. Eastburn A, Scherzer R, Zolopa AR, et al.. Association of low level viremia with inflammation and mortality in HIV-infected adults. PLoS One. 2011;6:e26320.
25. Lederman MM, Margolis L. The lymph node in HIV pathogenesis. Semin Immunol. 2008;20:187–195.
26. Dezube BJ, Lederman MM, Chapman B, et al.. The effect of tenidap on cytokines, acute-phase proteins, and virus load in human immunodeficiency virus (HIV)-infected patients: correlation between plasma HIV-1 RNA and proinflammatory cytokine levels. J Infect Dis. 1997;176:807–810.
27. Brenchley JM, Price DA, Schacker TW, et al.. Microbial translocation is a cause of systemic immune activation in chronic HIV infection. Nat Med. 2006;12:1365–1371.
28. Brenchley JM, Schacker TW, Ruff LE, et al.. CD4+ T cell depletion during all stages of HIV disease occurs predominantly in the gastrointestinal tract. J Exp Med. 2004;200:749–759.
29. Feng T, Wang L, Schoeb TR, et al.. Microbiota innate stimulation is a prerequisite for T cell spontaneous proliferation and induction of experimental colitis. J Exp Med. 2010;207:1321–1332.
30. Molina JM, Scadden DT, Amirault C, et al.. Human immunodeficiency virus does not induce interleukin-1, interleukin-6, or tumor necrosis factor in mononuclear cells. J Virol. 1990;64:2901–2906.
31. Gan HX, Ruef C, Hall BF, et al.. Interleukin-6 expression in primary macrophages infected with human immunodeficiency virus-1 (HIV-1). AIDS Res Hum Retroviruses. 1991;7:671–679.
32. Nakajima K, Martinez-Maza O, Hirano T, et al.. Induction of IL-6 (B cell stimulatory factor-2/IFN-beta 2) production by HIV. J Immunol. 1989;142:531–536.
33. Ambrosino C, Ruocco MR, Chen X, et al.. HIV-1 Tat induces the expression of the interleukin-6 (IL6) gene by binding to the IL6 leader RNA and by interacting with CAAT enhancer-binding protein beta (NF-IL6) transcription factors. J Biol Chem. 1997;272:14883–14892.
34. Rautonen J, Rautonen N, Martin NL, et al.. HIV type 1 Tat protein induces immunoglobulin and interleukin 6 synthesis by uninfected peripheral blood mononuclear cells. AIDS Res Hum Retroviruses. 1994;10:781–785.
35. Hoshino S, Konishi M, Mori M, et al.. HIV-1 Vpr induces TLR4/MyD88-mediated IL-6 production and reactivates viral production from latency. J Leukoc Biol. 2010;87:1133–1143.
36. Poli G, Bressler P, Kinter A, et al.. Interleukin 6 induces human immunodeficiency virus expression in infected monocytic cells alone and in synergy with tumor necrosis factor alpha by transcriptional and post-transcriptional mechanisms. J Exp Med. 1990;172:151–158.
37. Dandekar S, George MD, Baumler AJ. Th17 cells, HIV and the gut mucosal barrier. Curr Opin HIV AIDS. 2010;5:173–178.
This article has been cited 2 time(s).
Current Opinion in Hiv and AIDSSoluble biomarkers of HIV transmission, disease progression and comorbiditiesCurrent Opinion in Hiv and AIDS
Current Opinion in Hiv and AIDSStudy design issues in evaluating immune biomarkersCurrent Opinion in Hiv and AIDS
IL-6; HIV-1 RNA; histocultures; macrophages; LPS; flagellin
Supplemental Digital Content
© 2012 Lippincott Williams & Wilkins, Inc.
Highlight selected keywords in the article text.