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Factors limiting the efficacy of conventional antiretroviral therapy for HIV-1 infection include treatment adherence, pharmacokinetics and penetration into viral sanctuaries. These affect the rate of viral mutation and drug resistance. In attempts to bypass such limitations, nanoparticles containing ritonavir, indinavir and efavirenz (described as nanoART) were manufactured to assess macrophage-based drug delivery.
NanoART were made by high-pressure homogenization of crystalline drug with various surfactants. Size, charge and shape of the nanoparticles were assessed. Monocyte-derived macrophage nanoART uptake, drug release, migration and cytotoxicity were determined. Drug levels were measured by reverse-phase high-performance liquid chromatography.
Efficient monocyte-derived macrophage cytoplasmic vesicle uptake in less than 30 min based on size, charge and coating was observed. Antiretroviral drugs were released over 14 days and showed dose-dependent reduction in progeny virion production and HIV-1 p24 antigen. Cytotoxicities resulting from nanoART carriage were limited.
These results support the continued development of macrophage-mediated nanoART carriage for HIV-1 disease.
Although antiretroviral therapy (ART) has greatly reduced disease morbidity and mortality in HIV-1-infected people, a major limitation for treatment is the need for lifelong daily drug dosing. To achieve sustained viral suppression, maintenance of therapeutic drug levels is required [1–4]. Thus, suboptimal adherence causes increased risk for treatment failure and viral resistance . Moreover, penetration of drugs into viral tissue sanctuaries, such as the CNS, is also limited by oral ART, leading to diminished therapeutic efficacy reflected in cognitive dysfunction and accelerated disease [6–11]. In addition, substance abuse, common among HIV-1-infected individuals, has long been recognized as a risk factor for poor therapeutic adherence . As a result, healthcare providers are often reluctant to prescribe ART to patients who illicitly use drugs because of promotion of virologic resistance and accelerated viral transmission [13,14]. Adding to such concerns, ART is not yet available to all who need it, most notably those in resource-limited settings [15,16].
Thus, our laboratories have embarked on the development of nanoformulated ART aimed at virus target tissues and improved drug delivery. As monocytes and monocyte-derived macrophages (MDM) are cellular reservoirs for HIV and have the ability to uptake, transport and release ART into infected tissues, these cells were proposed as drug carriers [17–19]. Although such formulations were controlled for stability, early studies showed limitations in both cellular uptake and release, which necessitated ex vivo loading of monocytes and MDM followed by adoptive transfer in order to reach therapeutic end points. Indeed, the promise and perils for such nanotargets were reported previously in laboratory and animal models of human disease . With this in mind, we tested just such a drug-delivery approach adjusting for surfactant composition, size and charge. These enabled efficient development of nanoformulated antiretroviral drugs, collectively referred to as nanoART. Optimization of drug loading and release was done by pharmacokinetic and antiretroviral nanoART measurements. Cell entry and release of ritonavir (RTV), indinavir (IDV) and efavirenz (EFV) nanoparticles (NPs) were optimized based on size, coating and charge. Reverse-phase high-performance liquid chromatography (RP-HPLC) showed uptake of drugs into cells of 1 log or more or above the EC50 without cytotoxicity and sustained drug release for up to 15 days. Antiretroviral efficacy was determined by infecting MDM with HIV-1ADA (a macrophage tropic viral strain) every 5 days for up to 15 days following nanoART treatment. NanoART-loaded cells showed sustained antiretroviral activities for many of the formulations tested. These results provide proof-of-concept that ART compounds can be manufactured into stable NPs that can be targeted to cells and used in cell-mediated drug-delivery systems. These data also suggest that nanoART may be developed for human use to improve dosing schedule, optimize adherence and increase therapeutic efficacy for HIV-1 disease.
NanoART of IDV, RTV and EFV were prepared by high-pressure homogenization using an Avestin C-5 homogenizer (Avestin, Inc., Ottawa, ON, Canada). A range of surfactants were used to coat the drug crystals including Lipoid E80® (an egg phosphatide mixture of phosphatidylcholine, phosphatidylethanoloamine and the hydrolyzed lyso [single aliphatic chain]; Lipoid GmbH, Ludwigshafen, Germany), a block copolymer of ethylene oxide and propylene oxide (poloxamer 188 [P-188]; Spectrum Chemicals, Gardena, CA, USA), 1,2-distearoyl-phosphatidyl-ethanolamine-methyl-poly(ethylene-glycol) (DSPE-mPEG2000; Genzyme, Cambridge, MA, USA), poly(lactic-co-glycolic acid) (PLGA; ratio 50:50 of lactide to glycolide; Sigma-Aldrich, St Louis, MO, USA), (1-oleoyl-2-[6-[(7-nitro-2–1,3-benzoxadiazol-4-yl)amino]hexanoyl]-3-trimethylammonium propane) (DOTAP; Genzyme) and cetyltrimethyl ammonium bromide (CTAB; Sigma-Aldrich). To coat the nanosized drug crystals, either alone or in combination, each surfactant (or copolymer) (weight/weight percent) was made up of Lipoid E80 (1.4%), P-188 (0.5%), DSPE -mPEG2000 (0.2%), PLGA (12%), DOTAP (0.1%) and CTAB (0.5%). The nanosuspensions were formulated at a slightly alkaline pH of 7.8 using either 10 mM sodium phosphate or 10 mM HEPES as a buffer. Tonicity was adjusted with glycerin (2.25%) or sucrose (9.25%). Drug was added to the surfactant solution to make a concentration of approximately 2% (weight-to-volume ratio [%]). Lissamine rhodamine B 1,2-dihexadecanoyl-sn-glycero-3-phosphoethanolamine, triethylammonium salt (rDHPE; Invitrogen, Carlsbad, CA, USA) was used to label nanoART, which appeared as red fluorescence. In order to synthesize nanoART, a suspension was prepared by adding crystalline drug to a surfactant solution and mixing for 4–7 min using an Ultra-Turrax T-18 (IKA® Works Inc., Wilmington, NC, USA) rotor-stator mixer to reduce initial particle size. The suspension was homogenized at 20,000 pounds per square inch for approximately 30 passes or until desired particle size was reached. For DOTAP-containing suspensions, the homogenized suspension was centrifuged (12,100 × g for 30 min at 5°C) to pellet the drug particles. The supernatant was decanted and surfactant-containing DOTAP was added to the drug pellet. The drug was resuspended by mixing with an Ultra-Turrax T-18.
In the case of EFV–PLGA NPs, EFV (1.25 g) and PLGA (6 g) were dissolved in dichloromethane (50 ml) and added to a 1% poly(vinyl) alcohol solution (500 ml). Particle size was achieved by sonicating at 50% amplitude for 10 min using a 400/600 W sonicator with a ¾ inch high gain probe. The solution was stirred overnight to evaporate the dichloromethane-hardened particles. The suspension was then centrifuged, washed with 18-Ω water and decanted twice. The particles were suspended in 10% mannitol before being frozen or lyophilized for storage. For all nanosuspensions, particle size was measured using a HORIBA LA 920 light scattering instrument (HORIBA Instruments Inc., Irvine, CA, USA; RRI = 1.08 for IDV and 1.20 for RTV and EFV). ζ-potential was measured by diluting 0.1 ml of the suspension into 9.9 ml of 10 mM HEPES, pH 7.4 on a Malvern Zetasizer Nano series instrument (Malvern Instruments Inc., Westborough, MA, USA). Final drug content of the formulations was determined by RP-HPLC (data not shown).
Human monocytes were obtained by leukapheresis from HIV-1 and hepatitis seronegative donors and were purified by counter-current centrifugal elutriation . Wright-stained cytospins were prepared and cell purity assayed by immunolabeling with anti-CD68 (clone KP-1). Monocytes were cultivated at a concentration of 1 × 106 cells/ml at 37°C in a humidified atmosphere (5% CO2) in Dulbecco's modified Eagle medium supplemented with 10% heat-inactivated pooled human serum, 1% glutamine, 50 μg/ml gentamicin, 10 μg/ml ciprofloxacin and 1000 U/ml recombinant human macrophage colony stimulating factor, a generous gift of Wyeth Inc. (Cambridge, MA, USA). To induce differentiation to macrophages, monocytes were cultured for 7 days in the presence of macrophage colony stimulating factor .
Samples were fixed with 3% glutaraldehyde in 0.1 M phosphate buffer (pH 7.4) and further fixed in 1% osmium tetroxide in 0.1 M phosphate buffer (pH 7.4) for 1 h. Samples were dehydrated in a graduated ethanol series and embedded in Epon 812 (Electron Microscopic Sciences, Fort Washington, PA, USA) for scanning-electron microscopy. Thin sections (80 nm) were stained with uranyl acetate and lead citrate and observed under a transmission electron microscope (Hitachi H7500-I; Hitachi High Technologies America Inc., Schaumburg, IL, USA).
Monocyte-derived macrophages (2 × 106 per well) were cultured with nanoART at concentrations of 1, 10 and 100 μM. Uptake of nanoART was assessed without medium change for 24 h with cell collection occurring hourly. Adherent MDM were collected by washing three times with 1 ml of phosphate-buffered saline, followed by scraping cells into 1 ml phosphate-buffered saline. Samples were centrifuged at 950 × g for 10 min at 4°C, and the supernatant removed. Cell pellets were sonicated in 200 μl of methanol and centrifuged at 10,000 × g for 10 min at 4°C. The methanol extract was stored at −80°C until RP-HPLC analysis was performed.
After an initial 12 h exposure to nanoART, drug release from MDM with half media exchanges every other day was evaluated over a 2-week period. Media samples were saved along with replicate cells and stored at −80°C until RP-HPLC analysis could be performed using a modified version of a previously published method . Methanol-extracted cell suspensions were centrifuged at 21,800 × g at 4°C for 10 min. Media samples were thawed and deproteinated by the addition of methanol. The samples were centrifuged at 21,800 × g at 4°C for 10 min; supernatants evaporated to dryness under vacuum and were resuspended in 70 μl of 100% methanol. Triplicate 20 μl samples of processed media or cells were assessed by RP-HPLC using a YMC Pack Octyl C8 column (Waters Inc., Milford, MA, USA) with a C8 guard cartridge. Mobile phase consisting of 47% acetonitrile/53% 25mM KH2PO4, pH 4.15 (adjusted with 1 N HCl) was pumped at 0.4 ml/min with UV/Vis detection at 212 nm. For all antiretroviral drugs, quantitations were assessed by comparison to a standard curve of free drug (0.025–100 μg/ml) made in methanol.
Monocyte-derived macrophages were treated with 1, 10 or 100 μM of nanoART for 12 h, washed to remove excess drug and infected with HIV-1ADA at a multiplicity of infection of 0.01 infectious viral particles/cell  on days 1, 5, 10 and 15 after treatment. Following viral infection, cells were cultured for 10 days with half media exchanges every other day. Media samples were collected on days 5, 7 and 10 for measurement of progeny virion production, as assayed by RT activity . Parallel analyses for expression of HIV-1 p24 antigen by infected cells were performed by immunostaining on day 10 postinfection.
In a 96-well plate, media samples (10 μl) were mixed with 10 μl of a solution containing 100 mM Tris-HCl (pH 7.9), 300 mM KCl, 10 mM DTT, 0.1% nonyl phenoxylpolyethoxy-lethanol-40 and water. The reaction mixture was incubated at 37°C for 15 min and 25 μl of a solution containing 50 mM Tris-HCl (pH 7.9), 150 mM KCl, 5 mM DTT, 15 mM MgCl2, 0.05% nonyl phenoxylpolyethoxy-lethanol-40, 10 μg/ml poly(A), 0.250 U/ml oligo d(T)12–18 and 10 μCi/ml 3H-TTP was added to each well; plates were incubated at 37°C for 18 h. Following incubation, 50 μl of cold 10% TCA was added to each well, the wells were harvested onto glass fiber filters and the filters were assessed for 3H-TTP incorporation by β-scintillation spectropmetry using a TopCount NXT (PerkinElmer Inc., Waltham, MA, USA) .
Monocyte-derived macrophages were stained using Vybrant DiO cell-labeling solution and viable MDM were identified by green fluorescence. NPs were labeled with rDHPE by adding fluorescent phospholipid. rDHPE-labeled NPs (rDHPE-nanoART) exhibited a red fluorescence. Based on the amount of tracer added, the number of labeled phospholipid molecules represents a very small fraction of the total coating material and contributes minimally to the thickness of the phospholipid coating. This was confirmed by size measurements that showed no significant differences in the sizes of nanoART formulated with or without rDHPE phospholipid (data not shown). In addition, no differences were detected in the uptake or the release of drug formulated with the fluorescent phospholipid compared with unlabeled particles. For representative formulations tested, more than 95% of MDM had taken up rDHPE-nanoART after 12 h of incubation (data not shown). Images were captured every 30 s using a Nikon TE2000-U (Nikon Instruments Inc., Melville, NY, USA) with swept-field confocal microscrope 488 nm (green) and 568 nm (red) laser excitations, and a 60× objective.
Cells were fixed with 4% phosphate-buffered paraformaldehyde 10 days after HIV-1 infection. Mouse monoclonal antibodies to HIV-1 p24 (1:10, Dako, Carpinteria, CA, USA) were used to determine the density of HIV-1-infected cells. Quantification of immunostaining was performed by densitometry using Image-Pro Plus, v. 4.0 (Media Cybernetics Inc., Bethesda, MD, USA). Expression of p24 was quantified by determining the positive area (index) as a percentage of the total image area per microscopy field .
To determine any potential toxic effects of NPs on cells, monocytes and MDM were treated with 100 μM of NPs for 12 h, and cytotoxicity assessed over 24 h using alamarBlue™ assay (AbD Serotec, Raleigh, NC, USA) according to the manufacturer's instructions .
Monocyte migration across the blood–brain barrier was performed as previously described [24,25]. For this assay, 2 × 104 human brain microvessel endothelial cells (HBMECs) were seeded on collagen-coated FluoroBlok™ tinted tissue culture inserts (3 μm pore size) from BD Biosciences (Franklin Lakes, NJ, USA). Because HBMEC monolayers are not visible on these inserts, manual readings of trans-epithelial electric resistance were assessed with an EVOM voltmeter (World Precision Instruments, Sarasota, FL, USA) to confirm monolayer formation and confluence. Monocytes were labeled with calcein-AM (Invitrogen) at 5 μM/1 × 106 cells for 45 min and washed with phosphate-buffered saline. For migration, 2.5 × 105 labeled monocytes were placed on HBMEC monolayers (upper chamber of the FluoroBlok insert) and allowed to migrate across the monolayer for 2 h (37°C, 5% CO2). Monocytes migrating into the lower chamber were quantified using a fluorescence plate reader (absorbance: 494 nm; emission: 517 nm) and compared with a standard curve derived from a serial dilution of a known number of calcein-labeled cells.
Statistical Analysis Software (SAS Institute, Inc., Cary, NC, USA) was used for all data analyses. Data were collected on days 5, 7 and 10 for any drug by dose by challenge-day (drug*dose*chalday) combination, meaning a multivariate response format. Initially, we transformed this multivariate into a univariate response format. For the nanoART uptake, the nanoART release and the antiretroviral activity, we used the mixed procedure in statistical analysis software to assess the effects of drug*dose*chalday (fixed effects) on antiretroviral response and to estimate their least-squares means (lsmeans), while treating the experimental unit within drug by dose (experimental unit [drug*dose]) as random effect. The lsmeans obtained from the data analyses were normalized in consideration of the positive control (infected MDM without nanoART treatments). Outcome was expressed relative to expression by positive controls (HIV-1 infection but no nanoART treatment), outcome as 100%, and negative controls (no infection or nanoART treatment), outcome as 0%. The Student's t-test was used to test the differences between the means of percent RT activity for two formulations at the same concentration. A p-value of 0.05 or less was considered significant.
NanoART was manufactured as a nanosized drug crystal, prepared from free-base drug and coated with poloxamer and/or phospholipid surfactants with two notable exceptions. For EFV-2 and -3, the drug was first dissolved in a PLGA copolymer solution prior to NP preparation. For all, the physical properties of nanosuspensions differed substantively by size and charge (Table 1). The NP ζ-potential ranged from −34.0 mV for IDV-1 coated with Lipoid E80 to +15.5 mV for RTV-4 coated with DSPE-mPEG2000, P-188 and DOTAP. The average size ranged from 200 nm for RTV-2 to 1060 nm for IDV-1. A range of sized particles was observed from the nanometer to micrometer range (data not shown). NanoART suspensions showed distinctive morphologies based upon manufacturing methods, drug and surfactant coating. IDV, RTV and EFV NP preparations, over a range of particle sizes and surfactants, were either ellipsoid, rod, cuboidal or spherical in shape with smooth surfaces (Figure 1A, B, D, E, G & H). IDV NPs, over a range of sizes and surfactants, were ellipsoid in shape and had distinct smooth surfaces (Figure 1A & B). RTV NPs were rod-shaped prisms with sharp and geometrically varied edges (Figure 1D & E). The morphology of EFV NPs differed depending on the manufacture method. EFV-1 NPs, produced by high-pressure homogenization, were cuboidal with distinct, sharp and geometric edges (Figure 1G), while EFV-3 NPs, produced by sonication, were spherical with distinct and smooth surfaces (Figure 1H). Transmission-electron microscopy of MDM cocultured with IDV-4, RTV-4 and EFV-3 demonstrated NP co-localization in the MDM cytoplasm with retention of each formulation's structural integrity after uptake into cells and are readily identifiable based on their distinctive shapes (Figure 1C, F & I, colored outlines). No such structures were observed in transmission-electron microscopy of untreated MDM (data not shown).
Next, we determined the effect of altering individual physical properties of the NPs on MDM uptake. Using IDV as a representative drug formulation, we altered coating, size and charge of the nanoformulations and tested cell uptake and secretion profiles for each at a constant concentration of 100 μM. We determined the effect of surfactant coating on uptake by comparing IDV-1, which was coated with Lipoid-E80, to IDV-2, which was coated with a combination of P-188 and DSPE-mPEG2000 (Table 1). Significant differences (p < 0.05) were observed in uptake rate and drug concentration. Maximum uptake was observed at 8 h for IDV-1 and 12 h for IDV-2 (Figure 2A), and the absolute amount of intracellular IDV was 1.65-fold greater for IDV-2 (45.74 μg/1 × 106 cells) than for IDV-1 (27.71 μg/1 × 106 cells).
To substantiate the RP-HPLC findings, we assessed uptake kinetics in real-time by live confocal imaging. In these experiments, rDHPE-labeled nanoART were added to cultures containing green-labeled MDM. Sequential still images of live cells taken at timed intervals supported the drug uptake measures and also demonstrated that the cells were able to uptake IDV-2 at a much greater rate than IDV-1 (Figure 2B) (Supplementary videos 1 & 2; for full videos see online www.futuremedicine.com/toc/nnm/4/8). These data, taken together, show that both rate and absolute amount of nanoART uptake are affected by surfactant coating. Next, we determined the effect of particle size on MDM uptake by comparing IDV-2 (970 nm) to IDV-3 (430 nm), both coated with a combination of P-188 and DSPE-mPEG2000 (Table 1). Significant differences (p < 0.05) were seen in both rate and extent of uptake amongst these two formulations (Figure 2A). Maximum uptake was observed at 8 h for IDV-2 and 24 h for IDV-3. The absolute amount of intracellular nanoART was 2.56-fold greater for IDV-2 (45.74 μg/1 × 106 cells) than for IDV-3 (17.88 μg/1 × 106 cells). These data demonstrate that particle size affects the rate and absolute amount of NP absorption.
Finally, we determined the effect of particle surface charge by comparing the uptake of IDV-2 (−24.4 mV) and IDV-4 (+15.0 mV) (Table 1). The rate of uptake was similar for both formulations as was the time of maximum uptake, 8 h (Figure 2A). Differences in the absolute amounts of intra-cellular NPs for IDV-2 (45.74 μg/1 × 106 cells) and IDV-4 (53.78 μg/1 × 106 cells) are illustrated (Figure 2A). These data support the idea that size and surfactant are important parameters that dictate cell uptake. Moreover, during the first 4 h of exposure to nanoART, absorption varied depending on the physical properties of the different NP formulations (Figure 2B).
After verifying that alteration of the physical properties of IDV NPs affects MDM uptake, we determined whether these same parameters could be applied to EFV and RTV. Four different formulations of RTV were developed (Table 1). The RTV formulation with the slowest rate and lowest absolute amount of uptake was RTV-1, which was coated with DSPE-mPEG2000 alone, had a size of 200 nm and had a ζ-potential of −25.6 mV (Table 1). The RTV formulation with the fastest absorption rate and greatest accumulation of RTV was RTV-4, which was coated with a combination of P-188, DSPE-mPEG2000 and DOTAP, had a size of 620 nm and had a ζ-potential of +15.5 mV. Maximum uptake occurred at 8 h for RTV-4 and at 12 h for RTV-1. Absolute amount of uptake was approximately 1.5-times greater for RTV-4 (40.98 μg/1 × 106 cells) than for RTV-1 (24.68 μg/1 × 106 cells) (Figure 3). The physical properties of RTV-4 were similar to IDV-4. This suggests that the physical properties that optimize the uptake of IDV NPs also optimize the uptake of RTV NPs. Three different formulations of EFV were synthesized (Table 1). The EFV formulation with the poorest uptake was EFV-1, which was coated with P-188 and DSPE-mPEG2000, had a size of 600 nm and had a charge of −3.1 mV (Table 1). The formulation with the best uptake was EFV-3, which was encapsulated in PLGA, had a size of 300 nm, was coated with CTAB and had a charge of +7.4 mV (Table 1). Uptake of EFV-1 and -3 differed significantly in the absolute amount of uptake, but not in the rate (Figure 3). Maximum uptake occurred at approximately 1 h for both formulations. Absolute amount of uptake for EFV-3 (3.19 μg/1 × 106 cells) was three-times greater than for EFV-1 (0.91 μg/1 × 106 cells). On the other hand, EFV-3 had a different surfactant coating and was smaller in size when compared with IDV-4 and RTV-4, but had greater overall uptake when compared with EFV-1. This suggests that the physical properties that optimize the uptake of nanoART are drug dependent.
Diverse release profiles were seen for each drug and formulation. The amount of drug still contained within the cells and released into the media was assessed. We compared two representative formulations for each drug that were tested for NP uptake. When comparing MDM treated with either IDV-1 or IDV-4, the cellular drug content differed significantly (p < 0.05) at all time points (Figure 3). No drug was detectable by day 11 in cells treated with IDV-1 while drug was readily present at day 15 for IDV-4 (1.61 μg/1 × 106 cells). Drug concentration within media also differed significantly (p < 0.05) from days 3 to 15 (Figure 3). No drug was detectable in the media by day 13 in cells treated with IDV-1 while drug was readily present in IDV-4 treated MDM (16.37 μg/ml).
When comparing MDM treated with either RTV-1 or -4 the drug content of both the cells and the media differed (p < 0.05) at all time points (Figure 3). Drug was present within the cells at day 15 for both RTV-1 (0.19 μg/1 × 106 cells) and RTV-4 (8.69 μg/1 × 106 cells). Drug was also present within the media at day 15 for both RTV-1 (0.28 μg/ml) and RTV-4 (11.62 μg/ml). For MDM treated with either EFV-1 or -3 the drug content of both cells and media differed (p < 0.05) at all time points measured (Figure 3). No drug was detectable by day 7 in cells treated with EFV-1 while drug was present, albeit at low levels, at day 15 in cells treated with EFV-3 (0.09 μg/1 × 106 cells). At day 15, drug was present within the media from cells treated with EFV-3 (0.3 μg/ml), but by day 13 no drug was detectable from cells exposed to EFV-1.
Next, we assessed whether cell function was affected in monocytes and MDM loaded with nanoART. In these experiments, we used alamarBlue as a quantitative, scalable and rapid assay for cell viability and proliferation. The alamarBlue reagents incorporate an oxidation–reduction indicator that both fluoresces and changes color in response to chemical reduction of growth medium resulting from cell growth. Thus, the intensity of the oxidation–reduction indicator is proportional to cell growth and cell viability. Results show that each of the IDV NPs tested at the highest concentration used (100 μM) did not significantly change the viability of monocytes (Figure 4A) or MDM (Figure 4B). All RTV NP preparations also tested at 100 μM did not alter macrophage viability (Figure 4B) but decreased monocyte viability by 15% (Figure 4A). Although NP loading increased monocyte migration across artificial blood–brain barrier models for both IDV-4 and RTV-4, the increase was not statistically significant (Figure 4C).
To determine the in vitro antiretroviral effects of nanoART taken up by MDM, we treated cells with individual nanoART preparations at concentrations of 1, 10 and 100 μM for 12 h and challenged the cells with HIV-1ADA at a multiplicity of infection of 0.01 infectious virus particles/cell at 1, 5, 10 and 15 days after drug treatment. The same formulations at the same concentrations used for uptake and release were tested for antiretroviral activities to ensure that the data sets could be compared. A dose-dependent effect for RT activity for IDV-4 at all time points examined was observed, while IDV-1 exhibited a potential dose-dependent response only on days 1 and 5 (Figure 5A). When used at 100 μM, significant differences (p < 0.05) between the two formulations were observed starting on day 5 (Figure 5A). By day 15, IDV-1 treatment groups were not different from infected controls, while IDV-4 treatment groups maintained significant (p < 0.05) viral suppression (Figure 5A). Comparison of RT activity suppression activity for RTV-1 and -4 revealed potential dose–response trends for both drugs at all time points (Figure 5B). Reduced RT activity was maintained over time for cells treated with RTV-4 but not for cells treated with RTV-1. By day 15, RTV-1 showed a 34.84% reduction in RT activity compared with controls, while RTV-4 suppressed RT activity by 98.42% (Figure 5B). Comparison of EFV formulations yielded an apparent dose–response effect for EFV-3 on days 10 and 15 but not for EFV-1 (Figure 5C). Starting on day 5 and continuing through to day 15, significant differences (p < 0.05) between EFV-1 and -3 were seen at all treatment concentrations except for the 1 μM treatment group on day 15 (Figure 5C). By day 10 all treatment groups for EFV-1 were not significantly different from infected controls, while cells treated with 100 and 10 μM of EFV-3 induced significant (p < 0.05) viral suppression until day 15 (Figure 5C). Differences between total measured RT activities over 2 weeks are shown for cells treated with 100 μM of IDV-1, RTV-1 and EFV-1 compared with cells treated with the same concentration of IDV-4, RTV-4 and EFV-3 (Figure 5D & E).
Expression of HIV-1 p24 antigen was also used to substantiate antiretroviral activity in MDM that were treated with nanoART and subsequently infected with HIV-1. Evaluation of p24 expression by infected MDM treated with IDV-1 and IDV-4 showed a dose–response effect in the expression of p24 at all time points for cells treated with IDV-4 but only on day 1 for cells treated with IDV-1 (Figure 6). Significant differences (p < 0.05) between the two formulations were seen at all concentrations starting at day 1 (Figure 6). On day 15 cells treated with 100 μM of IDV-1 did not differ from infected controls, while those treated with 100 μM of IDV-4 showed significant differences (p = 0.0003) (Figure 6). Comparison of HIV-1 p24 antigen density in groups treated with RTV-1 or -4 showed potential dose–response effects at all time points for both formulations at all concentrations (Figure 6). Significant differences (p = 0.0156) in the density of HIV-1 p24 were observed starting on day 1 for cells treated with 100 μM of RTV NPs (Figure 6). By day 15, all treatment concentrations differed significantly between RTV formulations (p < 0.021) (Figure 6). When HIV-1 p24 expression was compared amongst groups treated with EFV-1 and -3, significant differences were seen at day 5 for cells treated with 10 μM of EFV nanoformulations (p = 0.0317) (Figure 6). By day 10, both formulations at all concentrations differed significantly (p < 0.0001) (Figure 6). While there was a gradual loss of viral inhibition by cells treated with EFV-1, viral suppression by cells treated with 100 μM of EFV-3 was maintained up to 15 days (p = 0.0001) (Figure 6). Overall, IDV-4, RTV-4 and EFV-3 inhibited HIV-1 progeny virion production in infected cells for 15 days, while IDV-1, RTV-1 and EFV-1 did not. This was demonstrated by the gradual loss of p24 inhibition as well as the breakthrough of viral spread over time as demonstrated by increased density of p24 labeling. This data set mirrors that of the RT analysis and demonstrates decreased rates of viral replication for IDV-4, RTV-4 and EFV-3 by showing reductions in both RT activity and HIV-1p24 over time.
The HIV-1 pandemic continues to grow. An estimated 33.2 million people globally are infected with the virus; 2.2 million deaths occurred in 2008 alone, with the majority coming from the resource-limited areas [15,16]. The requirement for uninterrupted daily dosing, suboptimal patient adherence and inadequate tissue penetration continue to lead to treatment failure in a proportion of patients receiving ART [1,26]. Thus, our research effort in ART delivery has focused on developing long-acting parenteral drug formulations that can be maintained inside cells for periods measured in weeks and that travel specifically to viral sanctuaries [17–19,27].
Using poorly water-soluble ART, we manufactured nanosuspensions by homogenization and/or sonication techniques, and studied, in a complete manner, the physical properties of nanoART including size, charge and surface coating. We now demonstrate that we are able to directly modify the pharmacokinetics and cellular handling of drugs by altering the physical properties of NP. Most importantly, we demonstrated proof of concept in that cells pretreated with nanoART release the drug and inhibit HIV-1 infection for up to 15 days after treatment.
Macrophage-based nanomedicine delivery has a number of advantages for ART in an infected human host, including drug stability, delivery into viral sanctuary sites and sustained release. First, oral administration of drugs shows limited biodistribution and commonly results in the development of viral sanctuaries. This can increase the rate of viral mutation, affect drug resistance and result in treatment failure [2–4]. In addition, inadequate penetration of ART drugs into the genital tract raises concern about the ongoing risk of transmission, even when plasma HIV RNA levels are below the limit of detection [28,29]. Second, once the NPs gain entry into the monocyte or MDM, the cells can hold the drug in an active and stable form for periods of weeks. As such, they could provide a means to improve dosing schedules, adherence to therapy and the therapeutic index. Third, since the very same cell that carries the virus throughout the body is being used to deliver drug, it is likely that suitable drug concentrations could reach tissue sites that otherwise would have little or no drug penetration. Indeed, we posit that such a drug-delivery system using highly stable nanoART specifically targeted to monocytes and macrophages could greatly improve therapeutic outcomes.
These studies are but an incremental advance from what is being realized for nanomedicine. Indeed, nanotechnology has revolutionized pharmacology and drug delivery [30–32]. NPs can be altered in size, shape and composition to allow incorporation of drugs with a variety of biochemical properties. In addition, formulating drugs as NPs can allow for cellular transport and delivery. MDM have been shown to be potential drug vehicles for uptake, transport and delivery of nanoART [17–19]. Based on known limitations, a broad range of methods was previously employed to incorporate ART drugs into nanocarriers, including mannosylated gelatin, squalenoyl NP, fullerene cages and polymeric nanogels [33–37]. However, in all cases, cellular uptake and release of the drug was either limited or complicated by toxicity. A recent report demonstrated that sustained plasma concentrations of ART could be achieved over weeks to months, but this required intramuscular or subcutaneous administrations . Indeed, in our own work, using intravenous routes of injection, the absolute level of cellular uptake and distribution hindered the system. Therefore, in vitro treatment with nanoART followed by adoptive transfer was required [17,18]. This poses a challenge concerning the use of nanoART in the clinic. In order to overcome this and other barriers, our laboratories have designed highly stable nanoART to specifically target monocytes and MDM, maximize cellular uptake and extend antiretroviral activity. Comparisons between results obtained in this cell-based system with in vivo drug distribution are currently ongoing in our laboratories.
The successful application of depot-injected risperidone in clinical practice demonstrated the benefits provided by long-acting drug therapies [39–42]. Risperidone is an example of a drug that successfully transferred from daily oral administration to a sustained depot injection. Similar to the present situation, depot injection of risperidone was a modification of a clinically accepted oral therapy. The use of this and other long-acting antipsychotic compounds improved dosing schedules, enhanced treatment adherence and improved treatment outcomes. We propose using nanoART for cell-based drug delivery to create a similar long-acting drug treatment for HIV infection. If nanoART could be manufactured to be stable, actively taken up by cells, transported into tissue and slowly released, then injectable long-acting antiretroviral nanoformulations, which we are in the process of developing, could be realized for translational studies.
Nanosized drug crystals coated with a mixture of surfactants enhanced cellular uptake and maximized time of drug release. By modifying the size, coating and charge of nanoART, we have determined important physical characteristics that greatly enhance the pharmacokinetics and cellular handling of nanoART. We determined that nanoART, which are approximately 1 μm in size, are taken up most rapidly. It has been shown that larger NPs are taken up in greater amounts by MDM compared with smaller particles [43–45]. This could potentially be due to the mechanism of uptake. Particles 1 μm or greater in size are generally taken up by phagocytosis, as opposed to smaller particles 300 nm or less, which are taken in by a pinocytotic-like mechanism such as clathrin/caveolae-mediated uptake [44,45].
We also determined that the surfactant used to coat nanoART greatly affects how cells handle them. It has been demonstrated that the coating of a NP can greatly affect cellular handling and stability [46–48]. In this study, a combination of DSPE-mPEG2000 and P-188 was optimal for IDV and RTV. However, EFV uptake and release was much greater when it was encapsulated with PLGA. This demonstrates that there may be an optimal single or combination of surfactants for each ART drug that best maximizes uptake and release by cells. We also determined that positively charged nanoART are taken up better than negatively charged ones; although the difference is slight, this parallels previous findings .
Most important was the demonstration of the antiretroviral potential of nanoART. Cells pretreated with nanoART were protected against viral challenge for up to 15 days. Not only can cells actively take up nanoART, but they can also maintain the particles for long periods of time and allow steady release of drugs in clinically significant amounts.
The data contained in this report take us one step closer to realizing our goal of the synthesis of long-acting, injectable nanoformulated ART for human use. The potential benefits of such therapies for patient compliance and improved disease outcomes are significant. Moreover, such a method of drug delivery could also limit many of the untoward side effects of ART currently seen with oral therapy. Overall, the maintenance of consistent therapeutic plasma drug concentrations, which could allow for simpler dosing schedules, reduce the rates of viral mutation and disease progression, combat virus in hidden sanctuaries and improve treatment adherence. Linking these observations to what can occur in vivo after nanoART parenteral injections remains the singular focus of our laboratories research pursuits.
The precise mechanisms of uptake and release of nanoART are being pursued. This would address questions on particle trafficking within the cell compartments and resolve the query of how nanoART can be maintained inside macrophages and secreted slowly over defined time periods. It would also determine whether there are subpopulations of macrophages that are more amenable to such cell carriage. The linkages between in vitro observations and in bivo pharmacokinetics, biodistribution and antiretroviral properties are required. This will ultimately translate the potential use of nanoART as a new drug-delivery system for HIV-1-infected people.
The authors thank R Taylor for critical reading of the manuscript and outstanding graphic and literary support. N Anderson's support for video editing and formatting is appreciated.
Financial & competing interests disclosure The work was supported by grants 2R01 NS034239, 2R37 NS36126, P01 NS31492, P20RR 15635, P01MH64570, and P01 NS43985 (to HE Gendelman) from the NIH and a grant from Baxter Healthcare in nanomedicine. S Graham, M Chaubal, J Werling and B Rabinow are employees of Baxter Healthcare Corporation who developed the nanoART formulations used in this article. The authors have no other relevant affiliations or financial involvement with any organization or entity with a financial interest in or financial conflict with the subject matter or materials discussed in the manuscript apart from those disclosed.
No writing assistance was utilized in the production of this manuscript.