Browse Subject Areas

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

  • Loading metrics

Efficacy of Carraguard®-Based Microbicides In Vivo Despite Variable In Vitro Activity

  • Stuart G. Turville,

    Current address: Center for Virus Research, Westmead Millennium Institute, Westmead Hospital and University of Sydney, Sydney, Australia

    Affiliation Center for Biomedical Research, HIV and AIDS Program, Population Council, New York, New York, United States of America

  • Meropi Aravantinou,

    Affiliation Center for Biomedical Research, HIV and AIDS Program, Population Council, New York, New York, United States of America

  • Todd Miller,

    Affiliation Center for Biomedical Research, HIV and AIDS Program, Population Council, New York, New York, United States of America

  • Jessica Kenney,

    Affiliation Center for Biomedical Research, HIV and AIDS Program, Population Council, New York, New York, United States of America

  • Aaron Teitelbaum,

    Affiliation Center for Biomedical Research, HIV and AIDS Program, Population Council, New York, New York, United States of America

  • Lieyu Hu,

    Affiliation Center for Biomedical Research, HIV and AIDS Program, Population Council, New York, New York, United States of America

  • Anne Chudolij,

    Affiliation Center for Biomedical Research, HIV and AIDS Program, Population Council, New York, New York, United States of America

  • Tom M. Zydowsky,

    Affiliation Center for Biomedical Research, HIV and AIDS Program, Population Council, New York, New York, United States of America

  • Michael Piatak Jr,

    Affiliation AIDS and Cancer Virus Program, SAIC-Frederick, Inc., National Cancer Institute, Frederick, Maryland, United States of America

  • Julian W. Bess Jr,

    Affiliation AIDS and Cancer Virus Program, SAIC-Frederick, Inc., National Cancer Institute, Frederick, Maryland, United States of America

  • Jeffrey D. Lifson,

    Affiliation AIDS and Cancer Virus Program, SAIC-Frederick, Inc., National Cancer Institute, Frederick, Maryland, United States of America

  • James Blanchard,

    Affiliation Tulane National Primate Research Center, Tulane University Health Sciences Center, Covington, Louisiana, United States of America

  • Agegnehu Gettie,

    Affiliation Aaron Diamond AIDS Research Center, Rockefeller University, New York, New York, United States of America

  • Melissa Robbiani

    Affiliation Center for Biomedical Research, HIV and AIDS Program, Population Council, New York, New York, United States of America

Efficacy of Carraguard®-Based Microbicides In Vivo Despite Variable In Vitro Activity

  • Stuart G. Turville, 
  • Meropi Aravantinou, 
  • Todd Miller, 
  • Jessica Kenney, 
  • Aaron Teitelbaum, 
  • Lieyu Hu, 
  • Anne Chudolij, 
  • Tom M. Zydowsky, 
  • Michael Piatak Jr, 
  • Julian W. Bess Jr


Anti-HIV microbicides are being investigated in clinical trials and understanding how promising strategies work, coincident with demonstrating efficacy in vivo, is central to advancing new generation microbicides. We evaluated Carraguard® and a new generation Carraguard-based formulation containing the non-nucleoside reverse transcriptase inhibitor (NNRTI) MIV-150 (PC-817). Since dendritic cells (DCs) are believed to be important in HIV transmission, the formulations were tested for the ability to limit DC-driven infection in vitro versus vaginal infection of macaques with RT-SHIV (SIVmac239 bearing HIV reverse transcriptase). Carraguard showed limited activity against cell-free and mature DC-driven RT-SHIV infections and, surprisingly, low doses of Carraguard enhanced infection. However, nanomolar amounts of MIV-150 overcame enhancement and blocked DC-transmitted infection. In contrast, Carraguard impeded infection of immature DCs coincident with DC maturation. Despite this variable activity in vitro, Carraguard and PC-817 prevented vaginal transmission of RT-SHIV when applied 30 min prior to challenge. PC-817 appeared no more effective than Carraguard in vivo, due to the limited activity of a single dose of MIV-150 and the dominant barrier effect of Carraguard. However, 3 doses of MIV-150 in placebo gel at and around challenge limited vaginal infection, demonstrating the potential activity of a topically applied NNRTI. These data demonstrate discordant observations when comparing in vitro and in vivo efficacy of Carraguard-based microbicides, highlighting the difficulties in testing putative anti-viral strategies in vitro to predict in vivo activity. This work also underscores the potential of Carraguard-based formulations for the delivery of anti-viral drugs to prevent vaginal HIV infection.


Education and condom use can help limit HIV-1 transmission [1][3], but as currently applied do not represent definitive solutions. Thus, additional strategies are required to stem the spread of infection [4]. Vaccine and microbicide strategies tested to date have not been successful [5][8]. In light of recent setbacks in vaccine research [9], there is an even greater need to identify alternative approaches that reduce the risk of acquiring HIV-1 infection. Microbicides, operationally defined as substances intended to reduce or prevent transmission of HIV and/or other sexually transmitted infections (STIs) when applied topically to genital mucosal surfaces (, represent one such option. While the efficacy of a topically applied microbicide is likely to depend on the timely and correct application of the product relative to potential exposure, the availability of such products still represents an important strategy that could help stem the spread of HIV-1. Experience with such products may also usefully inform the development of alternative, coitus independent strategies.

Development of current and future microbicides must take into account our cumulative knowledge of HIV transmission. The early events leading to HIV passage across the genital mucosa likely involves HIV capture by a wide variety of molecules on the surface of epithelial cells and/or leukocytes followed by infection of permissive target cells within the tissues. In vitro virus transmission models have shown that dendritic cells (DCs) can capture virus and efficiently transmit these virions to CD4 T cells across infectious synapses between DCs and T cells [10][14]. CCR5-using HIV (R5 HIV) can productively infect immature DCs, like those located at the body surfaces, with the newly produced viruses being readily transferred to T cells [15]. In addition, both immature and mature DCs can effectively internalize viruses and transfer these virions to T cells, in the absence of productive infection of the DCs [10][12], [14], [16][18]. It is likely that immediate capture of virus by mucosa-associated DCs then transmits the virus to CD4 T cells, where robust virus replication occurs [10], [15], [19], consistent with other evidence for a more dominant role for CD4 T cells in the subsequent amplification of virus [20][22]. Thus, we postulated that the ability of candidate compounds to block infection in DCs or DC-T cell co-cultures may provide a more rigorous and relevant in vitro evaluation of the capacity of potential microbicide formulations.

Microbicide strategies currently being explored include broad-acting formulations that block HIV attachment (e.g., Carraguard, Pro 2000, BufferGel), specific small molecule inhibitors that target viral or cellular molecules critical for virus attachment, entry, or fusion (e.g., CCR5 inhibitors, fusion inhibitors like T-1249, anti-envelope Abs), and anti-viral drugs (e.g., PMPA, TMC-120, UC-781, MIV-150) [23]. The appeal of the broad-acting compounds is that they should prevent HIV interactions with any cell type (independent of the molecules involved) while also potentially having activity against other STIs. Carraguard, is a representative of this group, and has been shown to have potent activity against X4 HIV isolates with more limited activity against R5 HIV isolates in vitro [24][30], as well as having activity against other STIs [31][36]. A recently completed Phase III efficacy trial testing the ability of Carraguard to prevent HIV infection in women revealed that Carraguard is safe and while the frequency of HIV infection was lower in the Carraguard arm (134 vs 151 seroconversions in the placebo group), this was not a statistically significant difference [8]. In addition to safety, the inherent rheological properties and stability profile of Carraguard renders it a promising formulation vehicle, which may also have some anti-viral activity, to which other anti-viral agents could be added to provide a more effective microbicide.

The aim of this study was to evaluate the capacity of a microbicide (PC-817) comprised of Carraguard and the non-nucleoside reverse transcriptase inhibitor (NNRTI) MIV-150 to inhibit DC-driven infection in vitro and prevent vaginal immunodeficiency virus infection in macaques. MIV-150 (developed by Medivir, AB, Sweden, and licensed to the Population Council) is a tight-binding NNRTI with a rapid association and slow dissociation rate, which has activity against a variety of HIV-1 isolates, as well as HIV-2 [37]. MIV-150 also has virucidal activity against cell-free HIV and its anti-viral activity is not affected by seminal fluid [37]. We provide the first evidence of the additive effects of Carraguard and MIV-150 against DC-mediated infections in vitro and demonstrate the efficacy of Carraguard-based gels and topically applied MIV-150 in vivo.

Materials and Methods

Cell culture and reagents: SUPT1/CCR5 CL.30 cells (provided by J. Hoxie, University of Pennsylvania) and 174×CEM cells (AIDS Research and Reagent Program, courtesy of Peter Cresswell) were maintained in RPMI 1640 (Cellgro; Fisher Scientific, Springfield, N.J.) with 10% (v/v) heat-inactivated fetal calf serum (FCS, Cellgro). The cell line (AIDS Research and Reagent Program, courtesy of Dr. John C. Kappes, Dr. Xiaoyun Wu and Tranzyme Inc) was maintained in DMEM (Cellgro) with 10% (v/v) heat-inactivated FCS. Peripheral blood mononuclear cells (PBMCs) were isolated from HIV seronegative leukocyte-enriched preparations purchased from the New York Blood Center using Ficoll-Hypaque density gradient centrifugation (Amersham Pharmacia Biotech, Uppsala, Sweden). Monocytes were isolated using CD14 magnetic cell sorting (Miltenyi Biotec, Auburn, CA), with washing and elution in cold 1× PBS supplemented with 1% AB human serum (Cellgro) and 1 mM EDTA (Sigma). Monocyte purity was verified in each experiment by CD14 (MP9) and CD3 (Leu-4) staining (both Becton Dickinson, San Jose, CA), with cut-off purities of 2% CD3 T cells. Monocytes were subsequently cultured in RPMI 1640 (Cellgro) containing 10 mM HEPES (GIBCO-BRL, Life Technologies, Grand Island, NY), 2 mM L-glutamine (GIBCO-BRL), 50 μM 2-mercaptoethanol (Sigma, St. Louis, MO), penicillin (100 U/ml)-streptomycin (100 μg/ml) (GIBCO-BRL), and 1% heparinized human plasma (Innovative Research, Southfield, MI) supplemented with 100 U/ml recombinant human interleukin-4 (IL-4) (R&D Systems, Minneapolis, MN) and 1000 U/ml recombinant human granulocyte-macrophage colony-stimulating factor (GM-CSF) (Biosource/Invitrogen, Carlsbad, CA). To generate mature DCs, day 5-cultured immature DCs were exposed to a maturation cocktail of IL-1β (10 ng/ml), IL-6 (1,000 U/ml), TNF-α (10 ng/ml) (all from R&D Systems, Minneapolis, MI) and PGE2 (1 μg/ml) (Sigma) for 48 hours. The phenotype of immature and mature DCs was routinely monitored by two-color flow cytometry using FITC-conjugated mouse Ab against HLA-DR (Becton Dickinson) combined with the following panel of phycoerythrin (PE)-conjugated mouse anti-human monoclonal Abs (MAbs): anti-CD25, -CD80, -CD86 (all Becton Dickinson), and -CD83 (PN IM2218; Immunotech, Marseille, France).

Microbicide preparations: Carraguard (Lot numbers 032805, 102505, 032906-A, 011005-B, and 010908) was prepared as a 3% (w/v) stock as described [34]. PC-817 (Lot numbers 032805, 102705, 040306-B, 011005, and 032707-A) was prepared adding a DMSO (Sigma) or ethanol solution of MIV-150 (Medivir AB, Sweden) to Carraguard, to a final concentration of 500 μM. 2.5% (25 mg/ml) methylcellulose (MC; Lot numbers 032805, 110205, 033006-A, 011005-A, 032807, and 011008) (Fisher) was used as a placebo vehicle control gel for the in vivo studies. To test the in vivo activity of MIV-150 alone, MIV-150 was mixed with 25 mg/ml MC (Lot numbers 040306-A, 032707B, and 011908). All gels were stored at room temperature. In vitro assays with MIV-150 were set up using 10 mM MIV-150 stocks dissolved in DMSO. 3% Carraguard stock solutions were diluted initially 1∶10 (v/v) with 1× PBS using a positive displacement pipette (Eppendorf, Hamburg, Germany).

Virus stocks and titering: HIVMN and HIVBal stocks were sucrose gradient purified lots #P3764 and #P3953 (courtesy of the AIDS and Cancer Virus Program, SAIC-Frederick, Inc., National Cancer Institute, Frederick, MD). The RT-SHIV construct is a hybrid of SIVmac239 bearing the reverse transcriptase gene derived from HIV HXB2 [38], [39]. RT-SHIV stocks for in vivo inoculations were grown in PHA activated human PBMCs (kindly provided by Disa Böttiger, Medivir AB, Sweden). RT-SHIV stocks were titered using the 174×CEM cell line and TCID50 was calculated according to the Reed and Muench formula.

For in vitro assays, a purified and high titer stock of RT-SHIV was generated as follows: 4 liters of viral supernatant were produced in the 174×CEM cell line and harvested over a period of 28 days. Viral supernatant was pre-cleared of cellular debris, by centrifugation at 1800×g for 30 min at 4°C using a benchtop centrifuge (Eppendorf). Virus was then concentrated 100 fold, using a Labscale tangential filter flow apparatus connected in parallel with two Pellicon XL 50 Cassettes with 1000 kDa molecular weight cut-off (Millipore, Billerica, MA). For 37 ml of virus filter concentrate, virus pellets were generated by ultracentrifugation in a SW28 rotor (Beckman-Coulter, Fullerton, CA) at 100,000 g through a 1 ml 20% glycerol cushion and then virus was resuspended in 400 μl of PBS and layered onto a 9 step 24% to 56% sucrose gradient. Virus was subsequently ultracentrifuged in a SW55Ti rotor (Beckman-Coulter) at 100,000×g for 3 hours with acceleration and deceleration set at 5 and 9 respectively. For sucrose gradients, peak viral fractions were harvested by analyzing A280 using a spectrophotometer and were later confirmed to correspond to peak infectivity using the cell line [15]. Harvested fractions were diluted 1 in 5 ml in 1× PBS and subsequently pelleted at 100,000×g for 90 min in a SW55 rotor (Beckman-Coulter). The pellets were resuspended overnight in 1 ml of PBS and stored at −80°C. The titer (2.49×108 TCID50/ml) was determined using 174×CEM cells as described above.

HIV/SIV infections and mature DC transfer assays: cells (plated at 5×103 cells/well in 96 well flat-bottomed plates 16 hours earlier) or PBMCs activated for 48 hours with 5 μg/ml PHA (Sigma) (106 cells/ml in 200 μl in 96 well round-bottomed plates) were treated with compounds for 30 min at 37°C and then challenged with 300 TCID50 of HIVBal or HIVMN or 600 TCID50 of RT-SHIV. Activated PBMCs were recultured with complete media supplemented with 10 U/ml of IL2(Roche). For immature and mature DCs, 1.5×105 cells (in 150 μl) were pretreated with compounds and pulsed with either 3000 TCID50 of HIVBal, 4500 TCID50 of RT-SHIV or 3000 TCID50 of VSVg pseudotyped, delta HIV envelope NL43 in 96 well V-bottomed plates (Corning, NY). After 2 hours at 37°C, mature DCs were washed 4 times in media and then 103 DCs were added to 5×103 indicator cells or 5×103 DCs were also added to equal numbers of either SUPT1/CCR5 CL.30 cells (for HIVBal) or 174×CEM cells (for RT-SHIV). Detection of virus transfer to cells was by X-gal staining as described [15], [40]. Detection of transfer to SUPT1/CCR5 CL.30 cells was by Q-PCR for HIV gag DNA and RT-SHIV transfer to 174×CEM cells was by Q-PCR for SIV gag DNA, as a function of cell numbers by using Q-PCR for albumin DNA [41], [42]. Virus-pulsed immature DCs were washed before being cultured in 96 well round-bottomed plates at 106 cells/ml in 200 μl of IL-4/GM-CSF media. Infection of immature DCs was monitored using intracellular stain for HIV gag p24 [43]. The percent inhibition of infection was calculated using the following equation:

Microbicide application and in vivo challenge: Adult female Chinese rhesus macaques (Macaca mulatta) were housed at the Tulane National Primate Research Center (TNPRC; Covington, LA). All studies were approved by the Animal Care and Use Committee of the TNPRC. Animal care procedures were in compliance with the regulations detailed in the Animal Welfare Act [44] and in the “Guide for the Care and Use of Laboratory Animals” [45]. All naïve animals tested negative for simian type D retroviruses, simian T cell leukemia virus-1, and SIV prior to use. Prior to virus challenge, animals received a single 30 mg i.m. injection of Depo-Provera. 35 days later, the macaques were sedated and 3 ml of compound were introduced atraumatically into the vaginal vault using a pliable French catheter. 1 ml of virus was applied 30 min later. At appropriate time points, pre and post viral challenge, animals were anesthetized with ketamine-HCl (10 mg/kg) prior to EDTA blood samples being taken (no more than 10 ml/kg/month/animal).

Anti-CD8 depletion: Monkeys were treated with the mouse-human chimeric anti-CD8 mAb cM-T807 (NIH Nonhuman Primate Reagent Resource-Beth Israel Deaconess Medical Center, Boston, MA), receiving 10 mg/ml s.c. at day 0, followed by 5 mg/kg i.v. on days 3, 7, and 10 [46]. To verify CD8 cell depletion, whole blood was stained according to the manufacturer's guidelines for phycoerythrin (PE)-conjugated anti-CD8 (clone DK25; BD Pharmingen), fluorescein isothiocyanate (FITC)-conjugated anti-CD4 (clone L200; Dako), peridinin-chlorophyll-Cychrome (PerCP-Cy5.5)-conjugated anti-CD3 (clone SP34; BD Pharmingen).

Plasma viral load: Plasma was collected from whole EDTA blood after bench top centrifugation (Eppendorf) at 800×g for 10 min. Contaminating platelets were removed by a second centrifugation at 800×g for 10 min. Plasma was then stored in 1 ml aliquots at −80°C until plasma viral load RNA detection. Measurement of plasma viral loads by quantitative RT-PCR was performed as previously described [47], [48]. We defined animals that were “infected” as those which recorded greater than 1000 RNA copies/ml in ≥2 samples post infection. Animals defined as “uninfected” had undectectable viral RNA for the duration of the viral challenge study (20 weeks) or <1000 RNA copies per ml at <2 time points post challenge.

ELISPOT assay: ELISPOT assays were performed as previously described [47], [49] using 300 ng p27/ml of AT-2 inactivated SIVmneE11S [50] (Lot# p3926, courtesy of the AIDS and Cancer Virus Program, SAIC-Frederick) as the SIV antigen (vs the no virus microvesicle controls). SIV-specific responses were determined by subtracting the responses detected in control cultures from those induced by AT-2 SIV. In each experiment, PBMCs were also cultured with 5 μg/ml Concanavalin A (Sigma) to control for PBMC functionality and assay integrity. Spots were counted using an AID ELISPOT reader (Cell Technology, Columbia, MD) with once optimized settings through all experiments and the mean (±SEM) numbers of spot forming cells (SFCs) from triplicate or duplicate cultures per animal were enumerated.

SIV specific antibody response: Plasma samples obtained were monitored for the presence of SIV envelope Abs by using an established ELISA protocol [51].

Whole blood CD8/CD4 T-cell counts: Absolute CD4 and CD8 cell counts were monitored by TruCount (BDBiosciences, Palo Alto, CA) staining of whole blood at the indicated time points.

Statistical analyses used in this study: Unless otherwise stated, data was tested for normal distribution using Origin software (Shapiro-Wilk test) (Originlab corporation, Northhampton, MA). For statistical comparisons, 2-tailed and paired t tests were used for the in vitro analyses. Fisher's Exact was calculated for in vivo analyses [52], with the aid of software published online at Standard p values <0.05 were taken as statistically significant.


Carraguard can inhibit or enhance infection in vitro

In order to evaluate a combined MIV-150/Carraguard formulation in macaques, it was necessary to use a virus isolate that was sensitive to the drug while also infectious in vivo. Consistent with the lack of activity of other NNRTIs against the reverse transcriptase of SIV, there was little or no in vitro activity of MIV-150 against wild type SIVmac239, SHIV-162P3, or SIVmac316 (data not shown). Thus, a chimeric RT-SHIV isolate expressing HIV-1 reverse transcriptase was chosen, which has been shown to be infectious in vivo and sensitive to MIV-150 [38].

The first aim was to compare the ability of Carraguard to block RT-SHIV versus HIV infection in standard in vitro assay systems. Using cells, HIVBal was inhibited by Carraguard in dose dependent manner over the viral titration, while Carraguard was ineffective against RT-SHIV at or below 6000 TCID50/ml (p>0.05, Fig. 1A). Surprisingly, there was a statistically significant increase in RT-SHIV infection (300–3000 TCID50/ml) in the presence of very low doses (∼2 µg/ml) of Carraguard (p<0.05). At higher virus inocula there were reductions in infections and this correlated with loss of the cellular integrity due to extensive viral cytopathic effect (evident upon microscopic examination). Titrated amounts of Carraguard were tested against sub-saturating doses of RT-SHIV vs HIVBal and HIVMN (Fig. 1B). As expected, the X4 HIVMN strain was potently inhibited in a dose-dependent manner (IC50 = 0.030 µg/ml±0.007; n = 3). In contrast, the HIVBal inhibition curve was non sigmoidal and Carraguard was two orders of magnitude less potent against this isolate (IC50 = 4.17 µg/ml±2.35; n = 3). RT-SHIV was not only three orders of magnitude less sensitive to Carraguard (IC50 = 27.39 µg/ml±6.77; n = 3) than HIVMN, but at amounts of <10 µg/ml of Carraguard there was evidence of enhancement (although this was not statistically significant, p>0.05).

Figure 1. Carraguard can inhibit or enhance cell-free infection.

(A) cells were exposed to 0–10 µg/ml of Carraguard, before graded doses of HIVBal or RT-SHIV were added. 24 h later, the media was replaced and cells were cultured for 4 d. The numbers of β-gal expressing SFCs per well are shown (mean±SD, triplicate cultures). (B) Titrated amounts of Carraguard were tested against of HIVMN (MN, up triangles), HIVBal (Bal) (down triangles), or RT-SHIV (circles) in the cell line as in (A). The data are shown as the percent inhibition (mean±SD, triplicate cultures) of infection in the test conditions relative to the no Carraguard control. Negative % inhibition values represent enhancement, with no inhibitor effect at 0%. (C) Titrated amounts of Carraguard were added to PHA activated PBMCs before the cells were cultured with Bal or RT-SHIV for 5 d. Infection was measured by Q-PCR. Data are shown for triplicate cultures (mean±SD). Data in (A–C) are representative of 3 independent experiments with different donors in each case.

To evaluate whether this enhancement was restricted to the cell line, activated PBMCs were treated with varying doses of Carraguard before being challenged with HIVBal or RT-SHIV. In contrast to the cell line, there was significant enhancement of infection with HIVBal below 10 µg/ml of Carraguard (p<0.02 for 2 µg/ml Carraguard vs the media control) and the enhancement of RT-SHIV was even more pronounced with significant levels of enhancement between 2 and 20 µg/ml (p<0.05 over this range) (Fig. 1C).

Carraguard enhances DC-mediated amplification of virus in T cells

Since DCs are so effective at capturing HIV [53], [54], it is likely that DC-driven dissemination and amplification of virus in CD4 T cells occurs at the mucosa in vivo [10], [42]. We set out to establish a robust, reproducible assay with which we could monitor putative microbicide formulations for their ability to prevent such DC-mediated virus spread. In every experiment we utilized mature DCs and compared CD4 T cell lines to the cells as the recipients, to control for donor specific-differences (in the recipient cells) and the data shown are representative of both co-culture methods.

Mature DCs readily transmitted both HIVBal and RT-SHIV to the recipient cells. Significant increases in the levels of infection were observed in the presence of 10 µg/ml of Carraguard (Fig. 2A; p<0.05 for 2×103–5×104 TCID50/ml of HIVBal and for 3×103–1.5×104 TCID50/ml of RT-SHIV). Using sub-saturating concentrations of virus, significant levels of enhancement were observed over Carraguard concentrations ranging from 2 to 50 µg/ml, with peak levels of enhancement occurring at 6 µg/ml for both viruses (Fig. 2B). The peak enhancement of RT-SHIV infection was significantly higher than that observed for HIVBal (p<0.04). To more closely dissect the mechanism of this enhancement, mature DCs were loaded with virus in the presence (Pre) or absence of Carraguard and then also included Carraguard in the DC/recipient co-cultures (Post; for those DCs not pre-treated with Carraguard). Enhancement of infection by the lower Carraguard doses was observed when it was present either during the virus pulse of the DCs (Pre) or during the DC/recipient cultures (Post) (Fig. 2C). The peak level of enhancement of RT-SHIV infection was not significantly different in either condition (p>0.05), although the peak enhancement of HIVBal infection was significantly greater for the pre-treated condition (p<0.01). Since increased conjugate formation between DCs and the recipient cells would enhance virus transmission and subsequent replication [55], the formation of conjugates was monitored in the presence of the low “enhancing” dose of Carraguard. However, the presence of 6 µg/ml of Carraguard, did not affect the percentages of mature DC-CD4 T cell conjugates (14.73%±2.12 vs 13.93%±2.18 for cells cultured in medium vs Carraguard for 24 h).

Figure 2. Carraguard augments mature DC-mediated amplification of infection.

(A) Mature moDCs were pre-incubated with 0, 10, or 200 µg/ml Carraguard and challenged with graded doses of Bal or RT-SHIV, washed, and co-cultured with cells. Mean SFCs (±SD, triplicate conditions) are shown from 1 of 4 experiments. (B) Carraguard-treated mature DCs were pulsed with Bal or RT-SHIV, washed, and co-cultured with cells as in (A). The percent inhibition of infection (mean±SD, triplicate conditions) is shown for 1 of 4 experiments. A statistically significant difference (p<0.05, two-tailed paired t-test) between the enhancement effects on Bal vs RT-SHIV infection is noted by the asterisk. (C) Mature DCs pre-treated with Carraguard (Pre, open squares) were challenged with 3000 TCID50 of Bal or 4500 TCID50 of RT-SHIV, washed, and co-cultured with cells. Alternatively, mature DCs were pulsed with virus, washed, added to cells and the graded doses of Carraguard added to the co-cultures (Post, filled squares). The percent inhibition (mean±SD, triplicates) are shown from 1 of 4 experiments. A statistically significant difference (p<0.01, two-tailed paired t-test) between the pre versus post Carraguard enhancement effects on Bal infection is noted by the asterisk.

Carraguard inhibits infection of immature DCs coincident with DC maturation

Given the unexpected result that low doses of Carraguard increased virus replication facilitated by mature DCs, the impact of Carraguard on infection of immature DCs was investigated. Monitoring immature DC infection in contrast to mature DC-mediated infection is important at several levels. Firstly, immature DCs in healthy non-inflamed mucosa are hypothesized to be one of the first leukocytes contacting HIV [14], [23], [56]. Secondly, the dynamic nature of DC interactions with CD4 T cells provides immature DCs the capacity to be highly efficient at viral transfer at low numbers over long periods of time [10], [19], [57], [58].

Carraguard potently inhibited HIVBal infection of immature DCs in a dose-dependent manner (Fig. 3A, IC50 = 1.61 µg/ml±0.21, n = 4), as detected by flow cytometry analysis of HIV p24 expression (since residual Carraguard interferes with the PCR assay). Upon examining the cultures it was apparent that the immature DCs were reacting to Carraguard; the cells rapidly adhered to the plates (within 2 hours) and then cell clustering (as seen with maturing DCs) was more apparent over time. In addition, cytokine profiles of immature DCs treated with increasing doses of Carraguard revealed production of TNF-α at doses greater than 50 µg/ml (data not shown). Flow cytometric analysis of Carraguard-treated DCs revealed a dose-dependent up-regulation of the DC maturation markers CD83 and CD86 (Fig. 3B). Knowing that DC maturation significantly impacts the levels of HIV replication, even when the stimulus is added after virus has been captured by the DCs [59], [60], we wanted to ascertain whether the Carraguard effect was acting at a later stage of the virus life cycle (and not necessarily at the level of virus capture or spread between cells). To do so, immature DCs were infected with VSVg envelope pseudotyped HIV NL43 delta envelope (VSV-HIV Δenv, which will not spread between cells), 16 hours later the cells were washed, and graded doses of Carraguard were added. As with HIVBal infection, Carraguard blocked VSV-HIV Δenv infection of immature DCs (Fig. 3A; IC50 = 1.61 µg/ml±0.21, n = 4 for both viruses). Because Carraguard was added 16 hours after the addition of virus and VSV-HIV Δenv would not spread between cells, the inhibitory capacity of Carraguard could not be associated with initial attachment and fusion.

Figure 3. Carraguard inhibits infection in immature DCs coincident with DC maturation.

(A) Immature DCs were pre-incubated with graded doses of Carraguard, after which the DCs were challenged with Bal (down triangles) or HIV Δenv pseudotyped with the VSVg envelope (Δenv, filled squares). Cells were harvested 5 d later and stained for (A) HIV capsid p24 protein (mAb KC-57-RD1) or (B) the surface maturation markers CD83 and CD86. (A) Percent inhibition (mean±SD, triplicates) of infection and (B) the MFIs (mean±SD of triplicates) of CD83 (black bar) and CD86 (grey bar) expression (on the entire DC population) are shown for 1 of 4 replicate experiments. CD83 and CD86 up-regulation in response to increasing doses of Carraguard correlate closely (r = 0.99). (C) p24 expression is plotted against CD83, showing the correlation between lower CD83 levels and HIV infection. Comparable results were obtained when comparing CD86 and p24 expression (data not shown).

To further correlate the maturation of immature DCs with inhibition of viral production, the appearance of the HIV p24 antigen was plotted against the mean fluorescence intensity (MFI) of the maturation marker CD83 (Fig. 3C). The appearance of CD83 negatively correlated with the expression of intracellular HIV p24 by DCs infected with either HIVBal or VSV-HIV Δenv (r = −0.86, p<0.03 and r = −0.91, p<0.02 for HIVBal and VSV-HIV Δenv, respectively; n = 4 for both viruses). Thus, the ability of the compound to inhibit viral replication in this setting appeared to be due to its ability to induce DC maturation.

The NNRTI MIV-150 overcomes Carraguard-mediated enhancement of infection

Preliminary in vitro studies examining the NNRTI MIV-150 (50 µM) and Carraguard in a combination formulation designated PC-815 revealed that combining these agents results in improved inhibitory effects against R5 clinical HIV-1 isolates and an HIV-2 isolate [37]. Knowing that blockade of DC-driven infection can require greater anti-viral drug potency to limit infection than is required in other in vitro assays [61], [62], we sought to determine the efficacy of a high dose (500 µM) MIV-150/Carraguard combination formulation designated PC-817 in our DC systems and in vivo.

Unlike Carraguard, MIV-150 potently inhibited infection of cells with HIVBal, RT-SHIV, and HIVMN at concentrations below 3 nM (HIVBal IC50 = 2.94 nM±1.20; RT-SHIV IC50 = 0.99 nM±0.10; HIVMN IC50 = 1.03 nM±0.27; n = 3 for each virus) (Fig. 4A). We attempted synergy analysis using the Chou-Talay algorithm as previously described [63], although both HIVBal and RT-SHIV inhibition/enhancement curves did not satisfy the basic assumptions of this type of analyses (i.e., the shape and potency of the Carraguard curves were different to the typical sigmoidal curve for MIV-150). Therefore, we restricted our studies to the ability of MIV-150 to overcome the enhancement observed in mature DC-driven RT-SHIV infection, the experimental system that was most significantly enhanced by Carraguard. Pre-treatment of DCs with either Carraguard or PC-817 and post-treatment with Carraguard resulted in comparable levels of enhancement of RT-SHIV infection, while addition of PC-817 to the DC/recipient mixtures (post-treatment) effectively inhibited virus replication (Fig. 4B). Thus, the presence of MIV-150 overcame the enhancing effects of Carraguard. To more closely examine the amounts of MIV-150 needed to overcome the Carraguard enhancement of infection, titrated doses of MIV-150 were added to mature DC/recipient mixtures in the presence of 2 µg/ml Carraguard. Less than 1 nM of MIV-150 partially reversed the enhancement by Carraguard, with complete inhibition of virus replication being observed in the presence of as little as 8 nM of MIV-150 (Fig. 4C, p<0.001).

Figure 4. MIV-150 overrides the augmentation of DC-driven infection by Carraguard.

(A) cells were pre-exposed to varying doses of MIV-150, challenged with the indicated viruses. Mean percent inhibition (±SD, triplicates) is shown from 1 of 3 experiments. (B) Mature DCs pre-treated with Carraguard (Carr Pre, open circles) or PC-817 (PC-817 Pre, open triangles; 33.3 nM MIV-150 per 2 µg/ml Carraguard) were pulsed with RT-SHIV, washed, and co-cultured with cells. Alternatively, mature DCs were pulsed with virus, washed, added to cells and the graded doses of Carraguard (Carr Post, filled circles) or PC-817 (PC-817 Post, filled triangles) added to the co-cultures. The concentrations indicated on the X axis indicate the Carraguard concentrations for each formulation. The percents of inhibition (mean±SD, triplicates) are shown for 1 of 3 similar experiments. (C) Mature DCs were treated with 2 µg/ml of Carraguard, pulsed with RT-SHIV, washed, and then cultured with cells in the presence (Carr+MIV-150) or absence (Carr) of varying doses of MIV-150 (nM). Percent inhibition of infection (mean±SD, triplicates) are shown for 1 of 3 identical experiments.

Carraguard-based gels inhibit immunodeficiency virus transmission in vivo

Concurrent with the in vitro research, in vivo studies were carried out in order to compare Carraguard and PC-817 for their ability to prevent vaginal RT-SHIV infection in macaques. Depo-Provera-treated macaques had 3 ml of the indicated gels applied vaginally and then varying doses of RT-SHIV were applied 30 min later. Doses of >3000 TCID50 of SIVmac239 (parental strain of RT-SHIV) were shown to be relatively high based on frequency of animal infections [64] and 300 TCID50 of SHIV162P3 is commonly used in testing other microbicide strategies [65], [66]. Therefore, we compared a similar low end dose of 103 TCID50 of RT-SHIV to two higher doses (104 and 105 TCID50), to more rigorously test the Carraguard-based gels. A 2.5% MC gel was used as the placebo to parallel the products used in the Phase III clinical trial [8]. Vaginal challenge with RT-SHIV infected animals in a dose-dependent manner, resulting in mean peak viremias of approximately 7.8×106, 2.8×106, and 1.5×106 SIV RNA copies/ml after challenge with 105, 104, and 103 TCID50, respectively (66.7%, 83.3%, and 46% infection in the MC-treated groups, Fig. 5). Analysis of the average area under the curve of the viral loads in the MC control groups, confirmed the correlation between the virus challenge dose and virus levels over time (weeks 1 to 16, r2 = 0.97).

Figure 5. Carraguard-based gels inhibit vaginal infection in macaques.

Depo-Provera-treated animals were treated with 3 ml of MC, Carraguard (Carr), or PC-817 30 min prior to challenge with 1 ml of or 103–105 TCID50 RT-SHIV. (A) Plasma viral loads were quantified by PCR and SIV gag RNA copies per ml of plasma are shown for each animal over time. The numbers of animals in the respective groups are indicated in each panel. Each symbol denotes a different animal (Table 1). (B) The frequencies (percentage of infected animals, mean±SEM) of infection in the MC, Carraguard, and PC-817-treated groups challenged with 103 and 104 TCID50 are plotted. Carraguard (p<0.02) and PC-817 (p<0.03) significantly reduced the frequency of immunodeficiency virus infection compared to the MC-treated placebo group.

Both Carraguard and PC-817 protected against vaginal RT-SHIV infection and this was dependent on the dose of challenge inoculum used (Fig. 5A). Neither gel protected against the 105 TCID50 dose of RT-SHIV, although the peak viral loads were delayed 1–2 weeks in 3 of the 4 Carraguard-treated animals and 2 of the 3 PC-817 treated animals compared to the infected MC-treated animals (Fig. 5A, bottom row). However, Carraguard and PC-817 reduced RT-SHIV infection at both the 104 and 103 TCID50 challenge doses (Fig. 5A, middle and top rows, respectively). The 2 PC-817-treated animals infected after the 104 TCID50 challenge showed typical plasma viremia peaking after 14 days, while the 1 Carraguard-treated animal infected after the 103 TCID50 challenge showed a delayed peak viremia compared to the MC-treated animals. Independent of the virus challenge dose and gel exposure, all animals that became infected with RT-SHIV (repeated positive samples) exhibited co-culture positivity and developed SIV-specific Ab and cellular responses, as expected (Table 1). One Carraguard-treated animal challenged with 104 TCID50 of RT-SHIV showed one low positive reading of <1000 copies/ml, but it was negative at all other time points. This animal did not appear to have developed adaptive SIV-specific responses that might have controlled infection (Table 1), suggesting that either innate responses controlled infection, that this was a false positive RNA result, or this was evidence of an abortive infection [67]. This was supported by the lack of the appearance of virus in the plasma after depletion of CD8 cells (for 2–3 weeks during which time increases in plasma virus levels were observed in positive control animals) using the mAb cM-T807 [68] (data not shown).

Due to the small sample size of each TCID50 challenge group, statistical analyses were performed on the combined data from the 103 and 104 TCID50 groups where there was at least some protective effect of the gels (Fig. 5B). Both Carraguard and PC-817 significantly inhibited infection (p<0.02 and p<0.03, respectively), reducing the frequency of infection to at least 75% of that seen in the MC-treated animals.

Activity of topically applied MIV-150 against RT-SHIV in vivo

Since PC-817 did not appear to exhibit any additional activity against vaginal RT-SHIV challenge above that seen with Carraguard, we examined the ability of MIV-150 in MC to limit vaginal spread. As predicted by the PC-817 data (Fig. 5), a single dose of 500 µM of MIV-150 in MC given 30 min prior to vaginal challenge with 103 or 104 TCID50 of RT-SHIV did not prevent infection, although the peak viremia was delayed by 1–2 weeks in all animals infected after challenge with 103 TCID50 and in one of the animals receiving the higher inoculum (Fig. 6A). However, repeated doses of 500 µM of MIV-150 (1.5 mM total) in MC given 24 h before, 30 min before, and 24 h after challenge did reduce RT-SHIV infection, delaying the peak viremia in 2 animals (Fig. 6B). Compared to the MC control where 5 of 6 (∼83%) animals challenged with 104 TCID50 became infected (Fig. 5A), only 3 of 7 (∼43%) animals receiving the 3 doses of MIV-150 in MC got infected and exhibited typical plasma viremias; MIV-150 reduced the frequency of normal infections by ∼49%. Surprisingly, 3 other animals were virus positive on repeated occasions after challenge, but their peak viremias were 3–4 logs lower than the placebo group, with virus ultimately becoming undetectable after 1.5–3 months. Unlike typically infected animals, CD8 depletion of these 3 animals with the abnormally low infection did not result in any rebound of plasma virus levels (Fig. 6C and D). Just like the one uninfected animal, these animals did not develop detectable SIV-specific Ab or T cell responses, which are observed in most infected animals (Table 1). Thus, topically applied MIV-150 can limit vaginal RT-SHIV infection.

Figure 6. In vivo activity of MIV-150-containing MC gels.

Depo-Provera-treated animals were treated with (A) 3 ml of MC containing 500 µM MIV-150 30 min prior to vaginal challenge with 103 or 104 TCID50 of RT-SHIV or (B) 3 ml of MC containing 500 µM MIV-150 24 h before, 30 min before, and 24 h after vaginal challenge with 104 TCID50 of RT-SHIV. Plasma viral loads over time are shown for the indicated numbers of animals in each group. One year after challenge the 3 animals with the low-level initial infection (now with undetectable virus) and two of the normally infected animals were treated with the anti-CD8 mAb to deplete CD8 cells. (C) Effective depletion of CD8 cells was verified by flow cytometry and the CD8 cells per µl of blood are shown for each animal. (D) Analysis of the plasma virus loads before during and after CD8 depletion, revealed no rebound in virus levels in the 3 animals with the unusual acute low-level infection. Each symbol denotes a different animal that are detailed in Table 1.


In vitro predictive indicators of potential microbicides are needed prior to any animal efficacy testing. Although which tests can predict in vivo efficacy is of much debate. The study herein, presents an extreme example where most in vitro results were discordant with those observed in vivo at several levels. For instance, based on in vitro data alone, there is little supporting evidence that Carraguard would be protective in vivo. Rather, significant levels of enhancement were observed in vitro with our challenge virus RT-SHIV when Carraguard levels were below 10 µg/ml in cell-free infections of cell lines and activated PBMCs and also in cell-associated assays where mature DCs were used to transfer to recipient cells. These enhancing effects were more pronounced than has been reported previously [37], probably due to the lower doses of gels employed herein, as well as the use of mature DC assays and/or differing viral strains. The only exception, in accord with the 103 and 104 TCID50 in vivo results, was the potent inhibition of immature DC infection. The latter is likely the result of indirect effects, as Carraguard also matured the DCs, and DC maturation is associated with the reduced capacity of viral production [16], [69][72], even when DCs receive the maturation stimulus after virus exposure [59], [60].

Considerable evidence has demonstrated that polyanions like Carraguard are significantly more effective against the positively charged X4 viruses [24][29]. There have also been some reports of polyanions enhancing infections on the basis of interactions with the V1/V2 regions of envelope [26], [27], [73]. Herein, it is apparent that the level of enhancement is also dependent on the R5 isolate used, being most pronounced with RT-SHIV in the mature DC/recipient co-cultures. The mechanism of in vitro enhancement remains unclear and cannot be attributed to the two main mechanisms needed for DC viral transfer: increased capture of virus by the DCs or increased DC-T cell conjugate formation. In contrast to the polyanion attachment inhibitor class, the NNRTI MIV-150 consistently was not only potent, but also very effective against the virus isolates used with this study. Importantly, MIV-150 also overcame the unsuspected enhancing effects of Carraguard in the mature DC/recipient mixtures. This supports the initial report showing the potent effects of Carraguard and MIV-150 in vitro against several R5 Clade C clinical isolates [37].

Based on these in vitro findings we would have predicted that Carraguard would exhibit limited efficacy in preventing R5 RT-SHIV infection in vivo, while the addition of MIV-150 to Carraguard would render PC-817 considerably more effective. This was, however, not the case and the in vivo data disagreed with most of the in vitro data at three levels. Firstly, Carraguard did not enhance infection in vivo. Secondly, Carraguard proved to be effective against relatively high dose challenges (103 and 104 TCID50) of RT-SHIV. Thirdly, due to the efficiency of Carraguard it was not possible to demonstrate any difference between Carraguard and PC-817, with them both reducing infection by at least 75% of that seen in MC placebo controls. This is not the first observation of discrepancies between in vitro and in vivo data. Several in vivo studies demonstrated that the level of the compound needed to prevent infection in vivo is several orders of magnitude higher than that seen in vitro [65], [74][76]. Although in all cases, investigators did not observe enhancement in vitro of their test compound prior to in vivo testing. Thus, the study herein presents a novel comparison where enhancement in vitro contradicted effective inhibition in vivo.

Understanding which variable(s) were dominant in vivo, may aid in the future design of in vitro assays to more consistently predict the potential outcomes in animal models and ultimately in humans. As in previous microbicide challenges in macaques [4], [65], [66], [76], [77], there is an inordinately large amount of compound being used topically relative to the test levels in vitro. The in vivo dose of Carraguard (30 mg/ml) is at least 300 fold higher than the maximum levels that can be used in vitro and more than 3000 fold higher than the doses at which in vitro enhancement was observed. This is largely due to the viscosity of the 30 mg/ml solution, which is necessary for it to remain in place in vivo, but which interferes with the in vitro assays. Complementing our immature DC infection data, in vitro studies using tissue explants demonstrated that Carraguard was able to reduce R5 HIVBal infection by 50%, even when it was used at only 3 mg/ml (10 fold less than the recommended in vivo dose) [78]. It is likely that Carraguard-based gels coat the epithelial surfaces providing a primary barrier against HIV entering the tissues and reaching the underlying leukocytes that would amplify infection. Only rare DC processes extending to the epithelial surface or breaks in the tissue caused by trauma or other infections would afford the gels direct access to the underlying DCs. Since immature DCs dominate in healthy epithelia, our data indicate that if Carraguard was to reach the cells it would limit infection of the immature DCs under these circumstances. As such, it is likely that the gel rarely encounters mature DCs and T cells in which the enhancing effects were observed in vitro. Importantly, there was no evidence of enhancement of infection in macaques when the gels were applied atraumatically 30 min prior to challenge. Having only ∼50% infection frequency in the control 103 TCID50 challenge group would have allowed the detection of any significant adverse enhancing effects of the gels if they had occurred. Analysis of macaque vaginal swabs within the first days after a single application of PC-817 (versus MC or nothing, 4 animals per group) revealed no change in the levels of cytokines or chemokines (Melissa Robbiani and Rachel Singer, unpublished observations). This suggests a lack of immunomodulation in vivo as reported recently in women [79]. There was no evidence of inflammation or enhancement of infection in the recently completed Phase III trial of Carraguard [8]. Furthermore, use of Carraguard 2–3 times a week has been reported to be acceptable and safe, affording no differences to the placebo-using couples [80] and daily use of Carraguard for 7–14 d was found to be safe in HIV-infected men and women [81].

Clearly, the outcome of the Phase III clinical trial is in opposition to the in vivo macaque data presented within, highlighting that challenges still lie ahead in the study design of animal models predicting efficacy in clinical trials. For instance, there are several variables that need to be considered in future animal trials. Firstly, the placebo control gels need to match the inherent rheological properties of the gel to be tested. The MC placebo used herein did not exactly match rheological properties of Carraguard, however MC was used in parallel in Phase III clinical trials and therefore cannot explain the contrasting observations in the animal studies presented herein. Secondly, the means by which the virus is introduced is also of importance, as the atraumatic application of cell-free virus in the macaque model diverges from that occurring in heterosexual HIV transmission in humans. Key variables in the latter situation are physical and sometimes traumatic (e.g., cultural practices such as dry sex) introduction of virus in the form of either a cell-associated or cell-free viral inocula in the presence of seminal fluid. The presence of seminal fluid as an additional variable may actually increase the effective viral inocula present, due to the presence of semen-derived amyloid fibrils [82]. However, Carraguard-based formulations show no limitations in activity in the presence of seminal fluid in vitro [37].

Inclusion of an additional agent that broadens the activity of a formulation (overcoming any potential limitations of the gel) is highly advantageous. To this end, extremely low doses of MIV-150 effectively inhibited infection and overcame any enhancing effects of Carraguard in vitro, suggesting that this would increase protection in vivo when comparing Carraguard versus PC-817. Unfortunately, improved efficacy of PC-817 over Carraguard in vivo could not be demonstrated, due to the potency of Carraguard under these conditions, probably as a result of Carraguard's strong barrier effect. Supporting this, we observed that a single 500 µM dose of MIV-150 in MC given 30 min prior to challenge was unable to protect against vaginal infection. However, the in vivo activity of topically applied MIV-150 was verified by the fact that repeated doses of MIV-150 in MC reduced vaginal infection. This possibly reflects the dosing and/or timing requirements for the activity of MIV-150 to be evident. Since MIV-150 has both anti-viral and virucidal activities, the need for higher doses could indicate the need for more drug to be absorbed into the tissues and/or that the virucidal effect is needed to limit spread, since more MIV-150 was needed for virucidal effects in vitro [37]. Ongoing macaque studies are exploring how MIV-150 is acting in vivo. These findings set the stage for future studies examining the repeated (e.g., daily) application of gels that would allow women to use them independent of coitus and macaque studies using Carraguard-based gels (with and without MIV-150), are underway. Also, the topical activity of the NNRTI MIV-150 indicates promise for alternative strategies employing anti-viral drug-containing microbicide vaginal rings.

These studies provide direct evidence that Carraguard-based gels can afford protection against immunodeficiency virus infection when they are applied before atraumatic cell-free virus exposure in the absence of seminal fluid. However, the lack of protection within the recent Carraguard clinical trial emphasizes how other variables in humans need to be addressed in future study design using macaques in microbicide testing. These include the viral inocula, the presence of seminal fluid, the challenge virus used, single versus multiple virus applications and inclusion of mechanical disruption that mimics coitus. Unfortunately, not all variables can be addressed in animal models. For instance, additional post-hoc survival analyses in the Phase III clinical trial of Carraguard based on behavior, other risk factors, and adherence levels revealed that HIV incidence continued to be lower in the Carraguard group among the women who used the gel during 100% of sex acts, although this also did not reach statistical significance (Robin Maguire, personal communication). Importantly, adherence to using the gel was a significant problem and it is not clear when the supposedly compliant women actually used the gel relative to sexual intercourse. It is quite likely that the window of opportunity for a gel to be effective when used as a single application will be narrower than that for repeated (e.g., daily) use, thereby further undermining the efficacy of a single dose product. In summary, the data herein demonstrate the efficacy of Carraguard-based gels at preventing vaginal infection in a controlled environment. Moreover, we provide the first evidence that topically applied MIV-150 can restrict vaginal RT-SHIV infection. Together, this sets the stage for future research on anti-HIV strategies (repeated gel applications, or long term drug release from vaginal rings) that would afford greater activity against HIV infection.


We thank Disa Böttiger (Medivir AB) for the original RT-SHIV stock and James Hoxie (University of Pennsylvania) for the SUPT1/CCR5 CL.30 cell line. The following reagents were obtained through the NIH AIDS Research and Reagent Program: 174×CEM cells, courtesy of Peter Cresswell and the cell line Dr. John C. Kappes, Dr. Xiaoyun Wu and Tranzyme Inc. We also wish to thank David Phillips for critical discussions and advice on producing Carraguard-based gel formulations and Robin Maguire for critical review of the manuscript. Finally, we thank the continued support of the veterinary staff at the TNPRC.

Author Contributions

Conceived and designed the experiments: SGT MR. Performed the experiments: SGT MA TM JK AT LH AC TZ MPJ JWB JB AG. Analyzed the data: SGT MA TM JK MPJ JWB JDL AG MR. Contributed reagents/materials/analysis tools: AT LH AC TZ MPJ JWB JDL JB AG. Wrote the paper: SGT MR. Significant editing of manuscript: JDL.


  1. 1. DiClemente RJ, Wingood GM, Harrington KF, Lang DL, Davies SL, et al. (2004) Efficacy of an HIV prevention intervention for African American adolescent girls: a randomized controlled trial. Jama 292: 171–179.
  2. 2. Gregson S, Garnett GP, Nyamukapa CA, Hallett TB, Lewis JJ, et al. (2006) HIV decline associated with behavior change in eastern Zimbabwe. Science 311: 664–666.
  3. 3. Stoneburner RL, Low-Beer D (2004) Population-level HIV declines and behavioral risk avoidance in Uganda. Science 304: 714–718.
  4. 4. Shattock RJ, Moore JP (2003) Inhibiting sexual transmission of HIV-1 infection. Nat Rev Microbiol 1: 25–34.
  5. 5. (2000) From the Centers of Disease Control and Prevention. CDC statement on study results of product containing nonoxynol-9. Jama 284: 1376.
  6. 6. Richardson BA (2002) Nonoxynol-9 as a vaginal microbicide for prevention of sexually transmitted infections: it's time to move on. Jama 287: 1171–1172.
  7. 7. van de Wijgert JH, Shattock RJ (2007) Vaginal microbicides: moving ahead after an unexpected setback. Aids 21: 2369–2376.
  8. 8. Skoler S, Ramjee G, Ahmed K, Altini L, Govender S, et al. (2008) Efficacy of Carraguard® for prevention of HIV infection among women in South Africa: a randomized, placebo-controlled trial. In preparation.
  9. 9. Kaiser J (2008) AIDS research. Review of vaccine failure prompts a return to basics. Science 320: 30–31.
  10. 10. Turville SG, Santos JJ, Frank I, Cameron PU, Wilkinson J, et al. (2004) Immunodeficiency virus uptake, turnover and two phase transfer in human dendritic cells. Blood 103: 2170–2179.
  11. 11. McDonald D, Wu L, Bohks SM, KewalRamani VN, Unutmaz D, et al. (2003) Recruitment of HIV and its receptors to dendritic-T cell junctions. Science 300: 1295–1297.
  12. 12. Wang JH, Janas AM, Olson WJ, Wu L (2007) Functionally distinct transmission of human immunodeficiency virus type 1 mediated by immature and mature dendritic cells. J Virol 81: 8933–8943.
  13. 13. McDonald D, Wu L, Bohks SM, KewalRamani VN, Unutmaz D, et al. Enhancement of HIV Infection by Dendritic Cells: Transfer of HIV to Target Cells Through an Infectious Synapse; 2003; Boston.
  14. 14. Wu L, KewalRamani VN (2006) Dendritic-cell interactions with HIV: infection and viral dissemination. Nat Rev Immunol 6: 859–868.
  15. 15. Turville SG, Aravantinou M, Stossel H, Romani N, Robbiani M (2008) Resolution of de novo HIV production and trafficking in immature dendritic cells. Nat Methods 5: 75–85.
  16. 16. Granelli-Piperno A, Delgado E, Finkel V, Paxton W, Steinman RM (1998) Immature dendritic cells selectively replicate M-tropic HIV-1, while mature cells efficiently transmit both M- and T-tropic virus to T cells. J Virol 72: 2733–2737.
  17. 17. Fahrbach KM, Barry SM, Ayehunie S, Lamore S, Klausner M, et al. (2007) Activated CD34-derived Langerhans cells mediate transinfection with human immunodeficiency virus. J Virol 81: 6858–6868.
  18. 18. Izquierdo-Useros N, Blanco J, Erkizia I, Fernandez-Figueras MT, Borras FE, et al. (2007) Maturation of Blood Derived Dendritic Cells Enhances HIV-1 Capture and Transmission. J Virol 81: 7559–7570.
  19. 19. Turville SG, Vermeire K, Balzarini J, Schols D (2005) Sugar-binding Proteins Potently Inhibit Dendritic Cell Human Immunodeficiency Virus Type 1 (HIV-1) infection and Dendritic Cell-directed HIV-1 Transfer. Journal of Virology 79: 13519–13527.
  20. 20. Zhang Z, Schuler T, Zupancic M, Wietgrefe S, Staskus KA, et al. (1999) Sexual transmission and propagation of SIV and HIV in resting and activated CD4(+) T cells. Science 286: 1353–1357.
  21. 21. Zhang ZQ, Wietgrefe SW, Li Q, Shore MD, Duan L, et al. (2004) Roles of substrate availability and infection of resting and activated CD4+ T cells in transmission and acute simian immunodeficiency virus infection. Proc Natl Acad Sci U S A 101: 5640–5645.
  22. 22. Haase AT (2005) Perils at mucosal front lines for HIV and SIV and their hosts. Nat Rev Immunol 5: 783–792.
  23. 23. Trapp S, Turville SG, Robbiani M (2006) Slamming the door on unwanted guests: why preemptive strikes at the mucosa may be the best strategy against HIV. J Leukoc Biol 80: 1076–1083.
  24. 24. Baba M, Snoeck R, Pauwels R, de Clercq E (1988) Sulfated polysaccharides are potent and selective inhibitors of various enveloped viruses, including herpes simplex virus, cytomegalovirus, vesicular stomatitis virus, and human immunodeficiency virus. Antimicrob Agents Chemother 32: 1742–1745.
  25. 25. Meylan PR, Kornbluth RS, Zbinden I, Richman DD (1994) Influence of host cell type and V3 loop of the surface glycoprotein on susceptibility of human immunodeficiency virus type 1 to polyanion compounds. Antimicrob Agents Chemother 38: 2910–2916.
  26. 26. Jagodzinski PP, Wierzbicki A, Wustner J, Kaneko Y, Kozbor D (1999) Enhanced human immunodeficiency virus infection in macrophages by high-molecular-weight dextran sulfate is associated with conformational changes of gp120 and expression of the CCR5 receptor. Viral Immunol 12: 23–33.
  27. 27. Moulard M, Lortat-Jacob H, Mondor I, Roca G, Wyatt R, et al. (2000) Selective interactions of polyanions with basic surfaces on human immunodeficiency virus type 1 gp120. J Virol 74: 1948–1960.
  28. 28. Bartolini B, Di Caro A, Cavallaro RA, Liverani L, Mascellani G, et al. (2003) Susceptibility to highly sulphated glycosaminoglycans of human immunodeficiency virus type 1 replication in peripheral blood lymphocytes and monocyte-derived macrophages cell cultures. Antiviral Res 58: 139–147.
  29. 29. Vives RR, Imberty A, Sattentau QJ, Lortat-Jacob H (2005) Heparan sulfate targets the HIV-1 envelope glycoprotein gp120 coreceptor binding site. J Biol Chem 280: 21353–21357.
  30. 30. Dezzutti CS, James VN, Ramos A, Sullivan ST, Siddig A, et al. (2004) In vitro comparison of topical microbicides for prevention of human immunodeficiency virus type 1 transmission. Antimicrob Agents Chemother 48: 3834–3844.
  31. 31. Zaretzky FR, Pearce-Pratt R, Phillips DM (1995) Sulfated polyanions block Chlamydia trachomatis infection of cervix- derived human epithelia. Infect Immun 63: 3520–3526.
  32. 32. Zacharopoulos VR, Phillips DM (1997) Vaginal formulations of carrageenan protect mice from herpes simplex virus infection. Clin Diagn Lab Immunol 4: 465–468.
  33. 33. Maguire RA, Zacharopoulos VR, Phillips DM (1998) Carrageenan-based nonoxynol-9 spermicides for prevention of sexually transmitted infections. Sex Transm Dis 25: 494–500.
  34. 34. Maguire RA, Bergman N, Phillips DM (2001) Comparison of microbicides for efficacy in protecting mice against vaginal challenge with herpes simplex virus type 2, cytotoxicity, antibacterial properties, and sperm immobilization. Sex Transm Dis 28: 259–265.
  35. 35. Buck CB, Thompson CD, Roberts JN, Muller M, Lowy DR, et al. (2006) Carrageenan is a potent inhibitor of papillomavirus infection. PLoS Pathog 2: e69.
  36. 36. Roberts JN, Buck CB, Thompson CD, Kines R, Bernardo M, et al. (2007) Genital transmission of HPV in a mouse model is potentiated by nonoxynol-9 and inhibited by carrageenan. Nat Med 13: 857–861.
  37. 37. Fernández-Romero JA, Thorn M, Titchen K, Sudol K, Li J, et al. (2007) Carrageenan/MIV-150 (PC-815), A Combination Microbicide. Sexually Transmitted Diseases 34: 9–14.
  38. 38. Uberla K, Stahl-Hennig C, Bottiger D, Matz-Rensing K, Kaup FJ, et al. (1995) Animal model for the therapy of acquired immunodeficiency syndrome with reverse transcriptase inhibitors. Proc Natl Acad Sci U S A 92: 8210–8214.
  39. 39. Balzarini J, Naesens L, Verbeken E, Laga M, Van Damme L, et al. (1998) Preclinical studies on thiocarboxanilide UC-781 as a virucidal agent. Aids 12: 1129–1138.
  40. 40. West JT, Weldon SK, Wyss S, Lin X, Yu Q, et al. (2002) Mutation of the dominant endocytosis motif in human immunodeficiency virus type 1 gp41 can complement matrix mutations without increasing Env incorporation. J Virol 76: 3338–3349.
  41. 41. Douek DC, Brenchley JM, Betts MR, Ambrozak DR, Hill BJ, et al. (2002) HIV preferentially infects HIV-specific CD4+ T cells. Nature 417: 95–98.
  42. 42. Frank I, Stoessel H, Gettie A, Turville SG, Bess JW Jr, et al. (2008) A fusion inhibitor prevents dendritic cell (DC) spread of immunodeficiency viruses but not DC activation of virus-specific T cells. J Virol 82: 5329–5339.
  43. 43. Lore K, Smed-Sorensen A, Vasudevan J, Mascola JR, Koup RA (2005) Myeloid and plasmacytoid dendritic cells transfer HIV-1 preferentially to antigen-specific CD4+ T cells. J Exp Med 201: 2023–2033.
  44. 44. Animal Welfare Act and Regulation Code of Federal Regulations T, Chapter 1, Subchapter A: Animals and Animal Products.
  45. 45. Guide for the Care and Use of Laboratory Animalspp. 1–83. Committee on Care and Use of Laboratory Animals of the Institute of Laboratory Animal Resources UDoHaHS (1985):.
  46. 46. Schmitz JE, Simon MA, Kuroda MJ, Lifton MA, Ollert MW, et al. (1999) A nonhuman primate model for the selective elimination of CD8+ lymphocytes using a mouse-human chimeric monoclonal antibody. Am J Pathol 154: 1923–1932.
  47. 47. Lifson JD, Rossio JL, Piatak M Jr, Parks T, Li L, et al. (2001) Role of CD8(+) lymphocytes in control of simian immunodeficiency virus infection and resistance to rechallenge after transient early antiretroviral treatment. J Virol 75: 10187–10199.
  48. 48. Cline AN, Bess JW, Piatak M Jr, Lifson JD (2005) Highly sensitive SIV plasma viral load assay: practical considerations, realistic performance expectations, and application to reverse engineering of vaccines for AIDS. J Med Primatol 34: 303–312.
  49. 49. Frank I, Santos JJ, Mehlhop E, Villamide-Herrera L, Santisteban C, et al. (2003) Presentation of exogenous whole inactivated simian immunodeficiency virus by mature dendritic cells induces CD4+ and CD8+ T cell responses. J AIDS 34: 7–19.
  50. 50. Lifson JD, Rossio JL, Piatak M Jr, Bess J Jr, Chertova E, et al. (2004) Evaluation of the safety, immunogenicity, and protective efficacy of whole inactivated simian immunodeficiency virus (SIV) vaccines with conformationally and functionally intact envelope glycoproteins. AIDS Res Hum Retroviruses 20: 772–787.
  51. 51. Smith SM, Holland B, Russo C, Dailey PJ, Marx PA, et al. (1999) Retrospective analysis of viral load and SIV antibody responses in rhesus macaques infected with pathogenic SIV: predictive value for disease progression. AIDS Res Hum Retroviruses 15: 1691–1701.
  52. 52. Agresti A (1992) A Survey of Exact Inference for Contegency Tables. Statistical Science 7: 131–135.
  53. 53. Frank I, Piatak MJ, Stoessel H, Romani N, Bonnyay D, et al. (2002) Infectious and whole inactivated simian immunodeficiency viruses interact similarly with primate dendritic cells (DCs): Differential intracellular fate of virions in mature and immature DCs. J Virol 76: 2936–2951.
  54. 54. Hu Q, Frank I, Williams V, Santos JJ, Watts P, et al. (2004) Blockade of Attachment and Fusion Receptors Inhibits HIV-1 Infection of Human Cervical Tissue. JExpMed 199: 1065–1075.
  55. 55. Pope M, Betjes MGH, Romani N, Hirmand H, Cameron PU, et al. (1994) Conjugates of dendritic cells and memory T lymphocytes from skin facilitate productive infection with HIV-1. Cell 78: 389–398.
  56. 56. Pope M, Haase AT (2003) Transmission, acute HIV-1 infection and the quest for strategies to prevent infection. Nature Medicine 9: 847–852.
  57. 57. Reece JC, Handley A, Anstee J, Morrison W, Crowe+ SM, et al. (1998) HIV-1 selection by epidermal dendritic cells during transmission across human skin. J Exp Med 187: 1623–1631.
  58. 58. Kawamura T, Cohen SS, Borris DL, Aquilino EA, Glushakova S, et al. (2000) Candidate microbicides block HIV-1 infection of human immature Langerhans cells within epithelial tissue explants. J Exp Med 192: 1491–1500.
  59. 59. Vachot L, Williams VG, Bess JW Jr, Lifson JD, Robbiani M (2008) Candida albicans-Induced DC Activation Partially Restricts HIV Amplification in DCs and Increases DC-to-T-Cell Spread of HIV. J AIDS 48: 398–407.
  60. 60. Trapp S, Derby N, Singer R, Shaw A, Williams VG, et al. (2008) The double stranded RNA analog poly(I∶C) inhibits HIV amplification in dendritic cells. Submitted.
  61. 61. Ketas T, Klasse P-J, Spenlehauer C, Nessin M, Frank I, et al. (2003) Inhibition of HIV-1 replication by the CCR5 antagonist SCH-C in multiple cell types. AIDS Res Hum Retroviruses 19: 177–186.
  62. 62. Ketas TJ, Frank I, Klasse P-J, Sullivan BM, Gardener JP, et al. (2003) Human immunodeficiency virus type 1 (HIV-1) attachment, coreceptor and fusion inhibitors are active against both direct and trans infection of primary cells. J Virol 77: 2762–2767.
  63. 63. Chou TC, Talaly P (1977) A simple generalized equation for the analysis of multiple inhibitions of Michaelis-Menten kinetic systems. J Biol Chem 252: 6438–6442.
  64. 64. McDermott AB, Mitchen J, Piaskowski S, De Souza I, Yant LJ, et al. (2004) Repeated low-dose mucosal simian immunodeficiency virus SIVmac239 challenge results in the same viral and immunological kinetics as high-dose challenge: a model for the evaluation of vaccine efficacy in nonhuman primates. J Virol 78: 3140–3144.
  65. 65. Veazey RS, Klasse PJ, Ketas TJ, Reeves JD, Piatak M Jr, et al. (2003) Use of a small molecule CCR5 inhibitor in macaques to treat simian immunodeficiency virus infection or prevent simian-human immunodeficiency virus infection. J Exp Med 198: 1551–1562.
  66. 66. Veazey RS, Shattock RJ, Pope M, Kirijan JC, Jones J, et al. (2003) Prevention of virus transmission to macaque monkeys by a vaginally applied monoclonal antibody to HIV-1 gp120. Nat Med 9: 343–346.
  67. 67. Miller CJ, Marthas M, Torten J, Alexander NJ, Moore JP, et al. (1994) Intravaginal inoculation of rhesus macaques with cell-free simian immunodeficiency virus results in persistent or transient viremia. J Virol 68: 6391–6400.
  68. 68. Schmitz JE, Kuroda MJ, Santra S, Sasseville VG, Simon MA, et al. (1999) Control of viremia in simian immunodeficiency virus infection by CD8(+) lymphocytes. Science 283: 857–860.
  69. 69. Canque B, Bakri Y, Camus S, Yagello M, Benjouad A, et al. (1999) The susceptibility to X4 and R5 human immunodeficiency virus-1 strains of dendritic cells derived In vitro from CD34(+) hematopoietic progenitor cells is primarily determined by their maturation stage. Blood 93: 3866–3875.
  70. 70. Bakri Y, Schiffer C, Zennou V, Charneau P, Kahn E, et al. (2001) The maturation of dendritic cells results in postintegration inhibition of HIV-1 replication. J Immunol 166: 3780–3788.
  71. 71. Cavrois M, Neidleman J, Kreisberg JF, Fenard D, Callebaut C, et al. (2006) Human immunodeficiency virus fusion to dendritic cells declines as cells mature. J Virol 80: 1992–1999.
  72. 72. Dong C, Janas AM, Wang JH, Olson WJ, Wu L (2007) Characterization of human immunodeficiency virus type 1 replication in immature and mature dendritic cells reveals dissociable cis- and trans-infection. J Virol 81: 11352–11362.
  73. 73. Crublet E, Andrieu JP, Vives RR, Lortat-Jacob H (2008) The HIV-1 envelope glycoprotein GP120 features four heparan sulfate binding domains, including the coreceptor binding site. J Biol Chem.
  74. 74. Tsai CC, Emau P, Jiang Y, Agy MB, Shattock RJ, et al. (2004) Cyanovirin-N inhibits AIDS virus infections in vaginal transmission models. AIDS Res Hum Retroviruses 20: 11–18.
  75. 75. Lederman MM, Veazey RS, Offord R, Mosier DE, Dufour J, et al. (2004) Prevention of vaginal SHIV transmission in rhesus macaques through inhibition of CCR5. Science 306: 485–487.
  76. 76. Veazey RS, Klasse PJ, Schader SM, Hu Q, Ketas TJ, et al. (2005) Protection of macaques from vaginal SHIV challenge by vaginally delivered inhibitors of virus-cell fusion. Nature 438: 99–102.
  77. 77. Lederman MM, Offord RE, Hartley O (2006) Microbicides and other topical strategies to prevent vaginal transmission of HIV. Nat Rev Immunol 6: 371–382.
  78. 78. Cummins JE Jr, Guarner J, Flowers L, Guenthner PC, Bartlett J, et al. (2007) Preclinical testing of candidate topical microbicides for anti-human immunodeficiency virus type 1 activity and tissue toxicity in a human cervical explant culture. Antimicrob Agents Chemother 51: 1770–1779.
  79. 79. Bollen LJ, Blanchard K, Kilmarx PH, Chaikummao S, Connolly C, et al. (2008) No increase in cervicovaginal proinflammatory cytokines after Carraguard use in a placebo-controlled randomized clinical trial. J Acquir Immune Defic Syndr 47: 253–257.
  80. 80. Kilmarx PH, Blanchard K, Chaikummao S, Friedland BA, Srivirojana N, et al. (2008) A randomized, placebo-controlled trial to assess the safety and acceptability of use of carraguard vaginal gel by heterosexual couples in Thailand. Sex Transm Dis 35: 226–232.
  81. 81. van de Wijgert JH, Braunstein SL, Morar NS, Jones HE, Madurai L, et al. (2007) Carraguard Vaginal Gel Safety in HIV-Positive Women and Men in South Africa. J Acquir Immune Defic Syndr 46: 538–546.
  82. 82. Munch J, Rucker E, Standker L, Adermann K, Goffinet C, et al. (2007) Semen-derived amyloid fibrils drastically enhance HIV infection. Cell 131: 1059–1071.