Search tips
Search criteria 


Logo of intjnanoDove Medical PressThis ArticleSubscribeSubmit a ManuscriptSearchFollowDovepressInternational Journal of Nanomedicine
Int J Nanomedicine. 2013; 8: 1417–1427.
Published online 2013 April 15. doi:  10.2147/IJN.S39888
PMCID: PMC3663477

Nanodiscs as a therapeutic delivery agent: inhibition of respiratory syncytial virus infection in the lung


There is increasing interest in the application of nanotechnology to solve the difficult problem of therapeutic administration of pharmaceuticals. Nanodiscs, composed of a stable discoidal lipid bilayer encircled by an amphipathic membrane scaffold protein that is an engineered variant of the human Apo A-I constituent of high-density lipoproteins, have been a successful platform for providing a controlled lipid composition in particles that are especially useful for investigating membrane protein structure and function. In this communication, we demonstrate that nanodiscs are effective in suppressing respiratory syncytial viral (RSV) infection both in vitro and in vivo when self-assembled with the minor pulmonary surfactant phospholipid palmitoyloleoylphosphatidylglycerol (POPG). Preparations of nanodiscs containing POPG (nPOPG) antagonized interleukin-8 production from Beas2B epithelial cells challenged by RSV infection, with an IC50 of 19.3 μg/mL. In quantitative in vitro plaque assays, nPOPG reduced RSV infection by 93%. In vivo, nPOPG suppressed inflammatory cell infiltration into the lung, as well as IFN-γ production in response to RSV challenge. nPOPG also completely suppressed the histopathological changes in lung tissue elicited by RSV and reduced the amount of virus recovered from lung tissue by 96%. The turnover rate of nPOPG was estimated to have a halftime of 60–120 minutes (m), based upon quantification of the recovery of the human Apo A-I constituent. From these data, we conclude that nPOPG is a potent antagonist of RSV infection and its inflammatory sequelae both in vitro and in vivo.

Keywords: nanodiscs, therapeutic delivery, anti-viral, innate immunity, phospholipids


Nanodiscs are self-assembled discoidal particles that are a phospholipid bilayer stabilized by an encircling helical protein “belt” called a membrane scaffold protein (MSP) (Figure 1).13 The MSP renders the entity soluble and biocompatible due to its amphipathic nature: non-polar residues face inward to mate with the acyl chains of the phospholipids, and polar/charged residues are at the aqueous interface. The MSP sequence was derived from the major protein component of the human high-density lipoprotein Apo A-I.411 While the primary circulating form of the high-density lipoprotein is a spherical particle with cholesterol esters in the core, its transitory, nascent form is discoidal.1214 A nanometer-scale membrane mimetic would have great utility in the investigation of biological processes involving membrane surfaces and associated membrane proteins. The necessity of obtaining homogeneous and monodisperse particles in order to apply the broad spectrum of biochemical and biophysical techniques to the study of integral membrane proteins assembled into nanodiscs required extensive protein engineering of the encircling Apo A-I protein. This effort resulted in a series of amphipathic helical MSPs that could be used to generate discoidal bilayer particles of varying size, currently ~9 nm to ~17 nm, where the length of the MSP determines nanodisc size.13 The resultant family of nanodiscs has seen broad application for the structural and functional studies of membrane proteins, following the discovery that detergent-solubilized membrane proteins could be self-assembled into the nanodisc by simple detergent removal with the target in a native-like lipid environment with “native structural presentation,” yet soluble in aqueous solutions.15,16 Numerous laboratories have taken advantage of nanodiscs, as has been summarized in recent reviews.1719 The human Apo A-I origin of MSPs suggests that nanodiscs could be useful for in vivo use as therapeutic delivery agents. In this communication, we demonstrate that nanodiscs can deliver therapeutic lipids to the lung, prevent viral infection, and suppress the ensuing deleterious inflammatory response.

Figure 1
Molecular dynamic simulated model of Nanodisc.30

Respiratory syncytial virus (RSV) is one of the most common pathogens affecting young children, with infection rates over 90% between birth and age two.20 There is also growing appreciation that RSV causes serious respiratory illness in the elderly and high-risk adults with chronic pulmonary diseases such as asthma and chronic obstructive pulmonary disease.21,22 There is currently no vaccine or clinically approved treatment for RSV infection.2022 Recent studies demonstrate that the minor pulmonary surfactant phospholipid, palmitoyloleoylphosphatidylglycerol (POPG), markedly attenuates RSV infection in vivo and in vitro.23 The primary action mechanism of POPG appears to be the inhibition of virus binding to epithelial cells.23 Unfortunately, there are limited means to deliver potentially therapeutic phospholipids in vivo, particularly to the alveolar compartment in the lung. Liposomes offer one potential vehicle, although many problems with formulation exist, including overall in vivo stability, preparation homogeneity, and the drug composition shelf-life. Nanodiscs can be generated with precise control over lipid content and particle size, can be lyophilized and reconstituted, and can be made pyrogen-free and antigenically neutral. In this study, we investigated the use of POPG nanodiscs as a means of introducing therapeutic lipids for the prevention of viral infection by RSV. We examined the potency and effectiveness of nPOPG as an antagonist of RSV infection using both in vitro and in vivo systems. We quantified the potency of nPOPG against RSV infection in vitro by measuring interleukin-8 (IL-8) production and viral plaque formation. In addition, we determined the effectiveness of nPOPG using a mouse model of RSV infection and estimated the stability of nPOPG in the lung. Our findings show the utility of nanodiscs as a therapeutic delivery platform and demonstrate the effective inhibition of RSV infection both in vitro and in vivo.


Virus preparation, cell culture, and RSV infection in vitro

The human RSV A2 strain was obtained from the American Tissue Culture Collection (VR-1540, Manassas, Virginia, USA). The virus was propagated in HEp2 cells (ATCC) with culturing in DMEM/F12 (Invitrogen, Camarillo, CA, USA), supplemented with 5% bovine growth serum (BGS; Hyclone, South Logan, UT, USA). RSV was purified using methods previously described, under endotoxin-free conditions.25,26 Viral titers and growth were measured by quantitative plaque assays, as previously described.23,27

Beas2B cells were obtained from ATCC and cultured using a BEBM-bronchial epithelial cell growth medium (Lonza, Walkersville, MD, USA). Cells were infected at a multiplicity of infection (MOI) of 0.5 and incubated for 48 hours. Phospholipids were obtained from Avanti (Alabaster, AL, USA). Prior to RSV infection, cells were pre-incubated with nPOPG and nPOPC (200 μg phospholipid/mL) for 1 h, with RSV subsequently added to the cultures. Beas2B cells were also stimulated with 10 ng/mL of the TLR5 agonist flagellin (Alexis Biochemicals USA, San Diego, California, USA), with or without liposome POPG, nPOPG, or nPOPC (200 μg phospholipid/mL) for 48 h. IL-8 release into the culture supernatants was determined by commercial ELISA assay (Invitrogen). The IC50 values for nPOPG were determined from the inspection of best-fit curves for the data points. The cytopathic effects of the cultures were examined by light microscopy.

Nanodisc preparation

The MSP used for self-assembling phospholipids into nanodiscs was expressed and purified as described previously1,2 For this work we used MSP1D1 with a heptahistidine N-terminal affinity tag, which forms nanodiscs with a diameter of 9.7 nm, containing approximately 125 POPC or POPG lipids per disc. Additional purification steps were used to reduce the endotoxin level of the protein preparation: the MSP preparation (100–150 mg) was adsorbed onto a 1 cm × 5 cm Ni-NTA column and washed with 10 bed volumes of an aseptically prepared 1% Triton X-100 solution in phosphate buffered saline (PBS), followed by 10 bed volumes of buffer without detergent. The MSP was eluted with a 0.3-M imidazole solution and the buffer exchanged using an Amicon15 centrifugal ultrafiltration concentrator. The sample was filter-sterilized and the endotoxin level determined using a PYROGENT-5000 assay (Lonza, Walkersville, MD, USA).

Nanodiscs composed of phospholipids and the scaffold protein MSP1D1 were prepared as previously described.1,2,17 Briefly, cholate-solubilized phospholipids and purified MSP1D1 were combined and sonicated to form clear solutions at molar ratios of 130:65:1 (cholate:POPC or POPG:MSP1D1). The cholate was removed from the preparations with Amberlite XAD-2. The sample integrity was confirmed by size-exclusion chromatography using a Superdex 200 10/300 GL column. In all samples, more than 95% of material was eluted as a single peak, with the retention time corresponding to a Stokes diameter of 9.7 ± 0.2 nm, which is consistent with previously published results.2

Measurement of mRNA-encoding RSV F-protein by qRT-PCR

HEp2 cells were cultured in 24-well plates and inoculated for 2 hours at 37°C with RSV at an MOI of 1 × 10−3, in either the absence or presence of 200 μg/mL nPOPG or nPOPC. Following the adsorption period the cells were washed three times with PBS and then shifted to a culture medium either with or without the nanodiscs. Immediately following adsorption, and at 24–96 hours, total well contents were processed for RNA extraction using a Qiagen RN-easy kit (Qiagen, Germantown, Maryland USA). The mRNA-encoding F-protein (F mRNA) was quantified using a qRT-PCR kit (Invitrogen). PCR products were also qualitatively analyzed by gel electrophoresis. The primers for F protein mRNA were 5′ GGAGGAAGTCTTAGCATATGTAG 3′ and 5′ CCATCCTCTGTCGGTTC 3′. We calculated gene expression levels using the manufacturer’s software (Bio-Rad Hercules, CA, USA).

Binding of RSV to epithelial cells

For cellular binding studies, HEp2 cells were grown in 24-well plates and RSV was adsorbed to the monolayers at varying MOIs (0, 1, 2, 5, and 10) for 2 hours at 18°C, either in the absence or presence of nPOPG, nPOPC, or liposome POPG (200 μg/mL of phospholipids). At 18°C, endocytosis by HEp2 cells is minimal, and this temperature allows viral binding to reach equilibrium within 2 hours.28 The cell monolayers were processed at 0°C for subsequent analysis by quantitative immunoblotting using a goat anti-RSV antibody (AbD Serotec, Raleigh, NC, USA).

In vivo measurements of nPOPG effects on RSV infection

Six-week-old female BALB/c mice were obtained from Jackson Laboratory (Bar Harbor, ME, USA). Mice were anesthetized and inoculated in a final volume adjusted to 50 μL. The RSV infection contained 1 × 107 pfu/50 μL in PBS. nPOPG was adjusted to 400 μg phospholipid in a total volume of 50 μL of PBS. For lipid antagonism, RSV and nPOPG were mixed together in PBS prior to inoculation. As described previously, all in vivo RSV effects required a replication-competent virus and were eliminated upon ultraviolet light inactivation of the virus.23 At 5 days after infection, mice were euthanized by intraperitoneal injection of 0.25 mL of Nembutal (10 mg/mL). All animal experiments followed prescribed guidelines and were approved by the Institutional Animal Care and Use Committee.

Euthanized mice were first dissected to expose the trachea and intubated with a cannula. The lungs were then lavaged with 1 mL of PBS. Next, the thorax was opened and the lungs were removed. The left lungs were homogenized in a DMEM tissue culture medium (Lonza, Walkersville, MD), and extracts were centrifuged at 2000 g for 15 minutes at 0°C and used for quantitative plaque assay analysis. Lower right lungs were fixed overnight in 10% buffered formalin, subsequently dehydrated and the tissues paraffin-embedded. Four-μm-thick sections were prepared and stained with Hematoxylin-Eosin. Tissues were evaluated using a histopathologic inflammatory scoring system, as described previously24 The lavage fluid was used for total cell counting, and differential cell counts were performed on cytospin preparations stained with trypan blue, as previously described.23 The cell-free supernatants resulting from the centrifugation of bronchoalveolar lavage fluid (BALF) were used for the measurement of IFN-γ by ELISA (BD Bioscience, San Diego, CA, USA).

Measurements of nPOPG turnover

Anesthetized mice were inoculated with 50 μL nanodisc preparations containing 400 μg of POPG. Following inoculation, the mice were euthanized at 0 minutes, 30 minutes, 60 minutes, 120 minutes, and 360 minutes. The euthanized mice were subjected to lavage with the thorax closed. Each animal received a 1-mL lavage of PBS. The recovered lavage material was subjected to SDS-PAGE and quantitative western blotting with an anti-Apo-A1 antibody (Calbiochem, La Jolla, CA, USA).

Statistical analysis

All results are shown as means ± SE. ANOVA was used to determine the level of difference between all groups. Differences were considered to be significant at P < 0.05.


nPOPG attenuates RSV-induced IL-8 production in human epithelial cells

IL-8 is produced by many types of epithelial cells in response to different infectious challenges and serves as an excellent biochemical marker for inflammatory processes. We compared the effects of nPOPG on RSV-induced IL-8 production in a human bronchial epithelial cell line (Beas2B). After 1 hour pre-incubation with either liposome POPG or nPOPG (both at 200 μg/mL phospholipid), Beas2B cells were infected with RSV at an MOI of 0.5 virus particles/cell for a period of 48 h. RSV infection induced a 100-fold increase in IL-8 production; liposome POPG inhibited this response by 95.4%, and nPOPG treatment suppressed this induction of IL-8 by 97.4% (Figure 2A). Liposomes and nanodiscs assembled with a control lipid, palmitoyloleoylphosphatidyl choline (POPC), which contains the same hydrophobic diacylglycerol moiety as POPG but differs in the hydrophilic head group, did not significantly inhibit IL-8 production. When Beas2B cells were challenged with the Toll-like receptor 5 ligand flagellin, they also produced a robust IL-8 response, but nPOPG, nPOPC, and liposome POPG were all ineffective at suppressing this inflammatory response (Figure 2B). These latter results demonstrate that the actions of nPOPG and liposome POPG are not non-specific, or cytotoxic, and do not generally suppress all inflammatory signaling pathways for the production of IL-8.

Figure 2
nPOPG inhibits RSV-induced IL-8 production by Beas2B cells. (A) IL-8 production by the Beas2B cells was measured by ELISA after either sham treatment or virus infection for 48 hours, in either the absence or presence of 200 μg/mL POPG, POPC added ...

For a more detailed comparison of the potency of nPOPG, we measured IL-8 production induced by the virus with varying doses of the lipid. The results from these experiments reveal that nPOPG exerts its effect in a concentration-dependent manner, with an IC50 of 19.1 ± 6.1 μg/mL and maximal inhibition at approximately 100 μg/mL (Figure 3A). Liposome POPG produces a similar IC50 at 12.3 ± 3.8 μg/mL. In contrast to nPOPG and liposome POPG, treatment with nPOPC at 200 μg/mL had a minimal inhibitory effect upon IL-8 production. Microscopic examination of the cytopathic effects of RSV is shown in Figure 3B. Control cells show a typical monolayer of Beas2B cells. Treatment with RSV added at an MOI of 0.5 for 48 h produces a cell layer with significantly reduced cell numbers, as well as cells with a hypertrophic, spindle-shaped morphology. Treatment of cells with RSV and nPOPC produces a cell layer that is quite similar in appearance to the virus-only treatment. In contrast, treatment of cells with RSV and nPOPG produces a cell monolayer that is nearly indistinguishable from control cells. Previously published micrographs also show that liposome POPG abrogates the cytopathic effects of RSV23 These data provide morphological evidence that POPG protects the epithelial cells from the cytopathic effects of RSV infection. From the above findings, we conclude that nPOPG is an effective antagonist of the RSV-induced inflammatory and cytopathic response of Beas2B cells.

Figure 3
Nanodisc POPG suppresses RSV-elicited IL-8 production in a concentration- and phospholipid class-dependent manner and inhibits the cytopathic effects of RSV upon Beas2B cells. (A) IL-8 production by Beas2B cells was measured by ELISA after challenging ...

nPOPG treatment inhibits RSV infection and in vitro plaque formation

We examined the ability of nPOPG to disrupt the RSV infection cycle by quantifying viral plaque formation with HEp2 cells in either the absence or presence of liposomes or nanodiscs reconstituted with POPG. Liposomes or nanodiscs were added 1 hour prior to the viral challenge, at a phospholipid concentration of 200 μg/mL. RSV, at titers of 2 × 104 − 2 × 10−2/mL, was allowed to adsorb to the cell monolayers for 1 hour with subsequent removal of the lipid and virus. These cultures were overlaid with agar and the formation of plaques was measured after 5 days. The liposome POPG inhibited plaque formation by >99% and the nPOPG attenuated plaque formation by 93% (Figure 4). These results show that nPOPG is effective as an in vitro inhibitor of RSV infection.

Figure 4
nPOPG inhibits RSV infection of HEp2 cells in tissue culture.

nPOPG interferes with viral propagation from the earliest stages of infection

Monolayers of HEp2 cells were infected at a low MOI, and the infection was followed for 4 days by using qRT-PCR to measure the mRNA encoding the viral F-protein. As shown in Figure 5, viral mRNA was detected after 24 hours of infection and continued to increase for another 72 hours. The inclusion of nPOPC with the RSV inoculum did not alter the growth of the virus. In contrast, the addition of nPOPG with the virus at the time of infection markedly suppressed the appearance and amount of viral RNA. At the end of the 96-hours growth period, the nPOPG-treated cultures expressed less than 1% of the RSV mRNA found in cells infected with the virus alone, or the virus plus nPOPC. These data demonstrate that nPOPG treatment markedly suppresses RSV gene expression and replication.

Figure 5
nPOPG inhibits the production of RSV mRNA. (A) Monolayers of HEp2 cells were pretreated with 200 μg/mL nPOPG or nPOPC for 1 h prior to the addition of RSV (multiplicity of infection = 1 × 10−3). After 2 h of RSV adsorption in the ...

nPOPG blocks RSV attachment to epithelial cells

To determine the site of nPOPG action as an antagonist of viral infection, we performed RSV binding experiments with monolayers of HEp2 cells in either the absence or presence of nPOPG, nPOPC, or liposome POPG. The attachment of the virus to the cell surface was quantified by recovering washed cell monolayers and performing electrophoresis and immunoblotting to detect viral proteins. The binding experiments were performed at 18°C to minimize endocytosis. The data in Figure 6A, show the immunoblot analysis of either uninfected cells or cells incubated with varying concentrations of virus, with or without nanodiscs or liposomes. The data in Figure 6B summarize the findings from three independent experiments. Virus attachment to the cell surface is a high-affinity saturable process. The addition of nPOPC to the binding reaction is without significant effect. In contrast, the inclusion of nPOPG suppresses RSV attachment to epithelial cells by 93% (at an MOI of 10), and liposome POPG inhibits this binding by 75% (at an MOI of 10).

Figure 6
nPOPG blocks RSV binding to epithelial cells. (A) Monolayers of HEp2 cells, at 18°C, were challenged with RSV at MOI = 0–10, as indicated, in either the absence or presence of 200 μg/mL nPOPC, nPOPG, or liposome POPG. UN identifies ...

Intranasal treatment of mice with nPOPG attenuates RSV infection in vivo

We utilized an in vivo infection model to examine RSV infection following intranasal administration of nPOPG. Mice were intranasally (1 × 107 pfu/mouse) inoculated with RSV, either in the absence or presence of liposome POPG or nPOPG containing 400 μg/mL phospholipid. Mice were euthanized 5 days after infection and their lungs were lavaged with 1 mL of saline. The recovered BALF was used for the analysis of total cell numbers, inflammatory cell populations, and IFN-γ production. The left lungs were harvested and processed for quantitative plaque assays to determine viral titers. The right lungs were processed for lung histology, and the degree of pathology was determined as previously described.23,24

As shown in Figure 7A RSV infection produced a 2.6-fold increase in the number of cells obtained by bronchoalveolar lavage when compared with sham-treated mice (CONL = 0.52 ± 0.1 × 105 cell/mL RSV = 1.31 ± 0.19 × 105 cell/mL). Liposome POPG and nPOPG treatment markedly reduced the total cells recovered in BALF after RSV infection (liposomes = 0.45 ± 0.04 × 105 cells/mL and nanodiscs = 0.56 ± 0.06 × 105 cells/mL). Inflammatory cell infiltrates induced by RSV consist mainly of neutrophils and lymphocytes, which are recovered in BALF. These inflammatory cell populations were significantly attenuated by treatment with liposome POPG and nPOPG, in conjunction with the RSV challenge (Figure 7B). IFN-γ production occurs as part of the host anti-viral response induced by RSV but is undetectable in uninfected animals. The robust IFN-γ response induced by RSV was completely eliminated in mice receiving either liposome POPG or nPOPG along with the virus (Figure 7C). The loss of the IFN-γ response occurring with nPOPG treatment is a result of lipid inhibition of the viral infection process. The production of infectious virus particles after the initial infection was quantified by performing plaque assays on lung homogenates. nPOPG suppressed the production of infectious particles by 97% and liposome POPG reduced this number by >99% (Figure 7D). In addition to sham-infected controls mice were treated with liposome POPG or nPOPG in the absence of virus (Figure 7AC). Mice given only liposome POPG or nPOPG did not show any significantly enhanced inflammatory cell migration into the lungs or increased IFN-γ production in the recovered BALF.

Figure 7
nPOPG inhibits RSV infection and inflammation in vivo. BALB/c mice were infected with RSV (1 × 107 pfu/mouse) by intranasal inoculation in either the absence or presence of liposome POPG or nPOPG (400 μg phospholipid), as indicated. The ...

We also examined the effects of nPOPG on lung histology, as previously described, for liposome POPG.23,24 The lung histology score of control animals was 2.1 ± 0.3, which was increased to 8.3 ± 0.7 by viral infection. As shown in Figure 8A, nPOPG reduced the virus effect on the histopathology score to 2.5 ± 0.5. In addition, treatment with nPOPG alone did not induce any inflammatory response. Figure 8B shows representative micrographs, which reveal the presence of lymphocytes and neutrophils in peribronchial and alveolar compartments in response to RSV infection. In contrast to the results obtained with RSV treatment alone, the inclusion of nPOPG with the virus almost completely suppressed the inflammatory histopathology. The histopathology results obtained with nPOPG are nearly identical to those previously reported for liposome POPG.23 In addition, treatment of the mice with nPOPG alone failed to produce evidence of significant inflammation in the tissue sections. Collectively, the above findings demonstrate that nPOPG is potent as a viral antagonist in mice.

Figure 8
nPOPG suppresses lung inflammation elicited by RSV. (A) Lungs from sham-infected (CONL) or RSV-infected mice treated with nPOPG were fixed in 10% buffered formalin, embedded in paraffin, and stained with hematoxylineosin. Lung sections from each animal ...

nPOPG turnover in the lung is rapid in vivo

We examined the in vivo turnover of nPOPG by measuring the amount of the MSP component of the nanodisc in BALF after intranasal inoculation. We inoculated 400 μg of nPOPG into mice and collected BALF at various time points and performed quantitative immunoblotting for MSP using a human Apo A-I antibody, as shown in Figure 9A. The time-dependent recovery of the Apo A-I was normalized to the initial amounts recovered immediately after inoculation. A strong Apo A-I signal was detected immediately following the inoculation and persisted through the 30-minutes and 1-hour time points. At 3 and 6 h after inoculation, the Apo A-I was either very low or undetectable in the mouse lavage. These results indicate a relatively rapid turnover for the nPOPG in mice and suggest a therapeutic window for nPOPG of approximately 1–2 hours in mice.

Figure 9
In vivo turnover of nPOPG in the lung. (A) Mice were anesthetized and inoculated with 400 μg nPOPG and euthanized at the indicated times. The euthanized animals were lavaged with one mL of PBS and the cell-free recovered material was subjected ...


In this report we provide evidence of an anti-inflammatory and anti-viral effect of nanodiscs assembled from MSP and the phospholipid POPG. In vitro studies revealed that nPOPG suppresses RSV-elicited IL-8 production with an IC50 of 19.3 μg/mL; this level is comparable to the value of 12.3 μg/mL obtained with liposomes. The findings demonstrate that nPOPG is effective at preventing the release of one of the earliest cytokines expressed by epithelial cells in response to viral infection. In vivo, IL-8 acts as a potent neutrophil chemotactic factor. The in vitro inhibition of viral plaque formation by nPOPG shows that concentrations of 200 μg/mL lipids suppress viral infection by 93%; this potency is nearly equivalent to that obtained with liposome POPG. This suppression of plaque formation is primarily a consequence of nPOPG inhibiting the attachment of the virus to the surface of epithelial cells. The in vitro viral binding experiments show that nPOPG is somewhat more effective than liposome POPG. Consistent with the findings that the viral attachment step is disrupted by nPOPG are the results demonstrating a reduction in viral F-protein mRNA production by a factor of 100.

The in vitro findings for nPOPG are also recapitulated in animal models of RSV infection. RSV challenges to mice demonstrate that 400 μg/mL nPOPG suppresses IFN-γ production and reduces the viral burden in the lung by 96%; similar effects are obtained with liposome POPG. The reduction of the in vivo IFN-γ response on day 5, near the peak of viral infection, clearly indicates that the viral infection has largely been unsuccessful. Consistent with this conclusion are the histopathological results demonstrating that nPOPG potently suppresses RSV-induced lung inflammation. The lack of significant increases in neutrophils in the lungs of mice treated with RSV and nPOPG indicates in vivo suppression of the production of keratinocyte chemoattractant, the mouse counterpart of IL-8. Collectively, these findings demonstrate that nPOPG has the potential to be a useful new type of drug delivery platform and an anti-viral agent against RSV, capable of significantly limiting infection and inflammation.

The Apo A-I content of nPOPG provides a convenient molecular marker for following the turnover of nanodiscs introduced into the lung by intranasal inoculation. Our results demonstrate that the apparent biological half-life for the protein component of the nanodiscs is between 60–120 min. This turnover rate indicates that nPOPG will only have a narrow window of efficacy in the mouse. However, the turnover of pulmonary surfactant proteins and lipids in the extracellular alveolar compartment is generally thought to be dependent upon the respiratory rate.29 In mice this respiratory rate is 250–300 breaths/min, whereas in humans this value is 18 breaths/minute in adults and 25–30 breaths/min in newborns. These differences in respiratory rate suggest that the turnover time of nPOPG may increase by as much as 10-fold in humans compared to mice. A turnover halftime of ~600 minutes in humans is a practical therapeutic window. The extracellular nPOPG action site requires that the extracellular pools of the lipid be maintained at adequate levels to prevent newly emergent viruses from spreading to the uninfected cells. Our experimental design utilized a single inoculation of nanodiscs in mice, as we wanted to avoid multiple rounds of anesthesia. Potential translation of the nPOPG system to humans might easily accommodate multiple dosing regimens within a 24-hour period. If higher levels of nPOPG can be maintained over longer time periods in humans, then such treatments should be effective for both prophylaxis and post-infection treatment.

Overall, our data show that nPOPG is comparable to liposome POPG in its anti-inflammatory and anti-viral properties. However, the nPOPG particles are ~10 nm × 5 nm in dimension and contain approximately 130 phospholipid molecules/particle, whereas the POPG liposomes are hollow spheres 25–50 nm in diameter that contain between 5 × 103 and 2 × 104 phospholipid molecules per particle. The smaller nanodisc size may offer some significant advantages for delivery to the lungs by inhalation. The MSP scaffold for nPOPG also provides a protein platform for modification that could potentially be manipulated to enhance the biological half-life or the targeting of the particles.

In summary, our data show that nanodiscs self-assembled with the therapeutic phospholipid POPG (nPOPG) effectively inhibit RSV infection and the resulting inflammatory response, both in vitro and in vivo. These findings suggest that nanodiscs may be a useful platform for the delivery of a range of bioactive lipids for therapeutic purposes.


This work was supported by NIH grant HL094629 and Colorado Bioscience Discovery Grant-2009 to DRV, and by NIH grants GM33775 and GM31756 to SGS.



The authors report no conflicts of interest.


1. Bayburt TH, Grinkova YV, Sligar SG. Self-assembly of discoidal phospholipid bilayer nanoparticles with membrane scaffold proteins. Nano Letters. 2002;2(8):853–856.
2. Denisov IG, Grinkova YV, Lazarides AA, Sligar SG. Directed self-assembly of monodisperse phospholipid bilayer nanodiscs with controlled size. J Am Chem Soc. 2004;126(11):3477–3487. [PubMed]
3. Grinkova YV, Denisov IG, Sligar SG. Engineering extended membrane scaffold proteins for self-assembly of soluble nanoscale lipid bilayers Protein Engineering. Design and Selection. 2010;23(11):843–848. doi: 10.1093/protein/gzq060. [PMC free article] [PubMed] [Cross Ref]
4. Atkinson D, Small DM. Recombinant lipoproteins: implications for structure and assembly of native lipoproteins. Annu Rev Biophys Biophys Chem. 1986;15:403–456. [PubMed]
5. Atkinson D, Smith HM, Dickson J, Austin JP. Interaction of apoprotein from porcine high-density lipoprotein with dimyristoyl lecithin. 1. The structure of the complexes. Eur J Biochem. 1976;64(2):541–547. [PubMed]
6. Brouillette CG, Anantharamaiah GM, Engler JA, Borhani DW. Structural models of human apolipoprotein A-I: a critical analysis and review. Biochim Biophys Acta. 2001;1531(1–2):4–46. [PubMed]
7. Brouillette CG, Jones JL, Ng TC, Kercret H, Chung BH, Segrest JP. Structural studies of apolipoprotein A-I/phosphatidylcholine recombinants by high-field proton NMR, nondenaturing gradient gel electrophoresis, and electron microscopy. Biochemistry. 1984;23(2):359–367. [PubMed]
8. Jonas A. Reconstitution of high-density lipoproteins. Methods Enzymol. 1986;128:553–582. [PubMed]
9. Matz CE, Jonas A. Micellar complexes of human apolipoprotein A-I with phosphatidylcholines and cholesterol prepared from cholate-lipid dispersions. J Biol Chem. 1982;257(8):4535–4540. [PubMed]
10. Segrest JP. Amphipathic helixes and plasma lipoproteins: thermodynamic and geometric considerations. Chem Phys Lipids. 1977;18(1):7–22. [PubMed]
11. Wlodawer A, Segrest JP, Chung BH, Chiovetti R, Jr, Weinstein JN. High-density lipoprotein recombinants: evidence for a bicycle tire micelle structure obtained by neutron scattering and electron microscopy. FEBS Lett. 1979;104(2):231–235. [PubMed]
12. Fielding CJ, Fielding PE. Dynamics of lipoprotein transport in the circulatory system. In: Vance DE, Vance JE, editors. Biochemistry of Lipids, Lipoproteins and Membranes. 5th ed. Amsterdam: Elsevier; 2008. pp. 533–553.
13. Zannis VI, Chroni A, Krieger M. Role of apoA-I, ABCA1, LCAT, and SR-BI in the biogenesis of HDL. J Mol Med (Berl) 2006;84(4):276–294. [PubMed]
14. Marcel YL, Kiss RS. Structure-function relationships of apolipoprotein A-I: a flexible protein with dynamic lipid associations. Curr Opin Lipidol. 2003;14(2):151–157. [PubMed]
15. Nath A, Atkins WM, Sligar SG. Applications of phospholipid bilayer nanodiscs in the study of membranes and membrane proteins. Biochemistry. 2007;46(8):2059–2069. [PubMed]
16. Sligar SG. Finding a single-molecule solution for membrane proteins. Biochem Biophys Res Commun. 2003;312(1):115–119. [PubMed]
17. Ritchie TK, Grinkova YV, Bayburt TH, et al. Reconstitution of membrane proteins in phospholipid bilayer nanodiscs. Methods Enzymol. 2009;464:211–231. [PubMed]
18. Bayburt TH, Sligar SG. Membrane protein assembly into nanodisks. FEBS Letters. 2010;584(9):1721–1727. [PubMed]
19. Denisov IG, Sligar SG. Cytochromes P 450 in nanodiscs. Biochim Biophys Acta. 2011;1814(1):223–229. [PMC free article] [PubMed]
20. Simoes EA. Respiratory syncytial virus infection. Lancet. 1999;354(9181):847–852. [PubMed]
21. Falsey AR, Hennessey PA, Formica MA, Cox C, Walsh EE. Respiratory syncytial virus infection in elderly and high-risk adults. N Engl J Med. 2005;352(17):1749–1759. [PubMed]
22. Hall CB. Respiratory syncytial virus and parainfluenza virus. N Engl J Med. 2001;344(25):1917–1928. [PubMed]
23. Numata M, Chu HW, Dakhama A, Voelker DR. Pulmonary surfactant phosphatidylglycerol inhibits respiratory syncytial virus-induced inflammation and infection. Proc Natl Acad Sci USA. 2010;107(1):320–325. [PubMed]
24. Cimolai N, Taylor GP, Mah D, Morrison BJ. Definition and application of a histopathological scoring scheme for an animal model of acute Mycoplasma pneumoniae pulmonary infection. Microbiol Immunol. 1992;36(5):465–478. [PubMed]
25. Dakhama A, Park JW, Taube C, et al. The enhancement or prevention of airway hyperresponsiveness during reinfection with respiratory syncytial virus is critically dependent on the age at first infection and IL-13 production. J Immunol. 2005;175(3):1876–1883. [PubMed]
26. LeVine AM, Elliott J, Whitsett JA, et al. Surfactant protein-D enhances phagocytosis and pulmonary clearance of respiratory syncytial virus. Am J Respir Cell Mol Biol. 2004;31(2):193–199. [PubMed]
27. McKimm-Breschkin JL. A simplified plaque assay for respiratory syncytial virus – direct visualization of plaques without immunostaining. J Virol Methods. 2004;120(1):113–117. [PubMed]
28. Numata MKP, Nagashima Y, Posey J, Hartshorn K, Woodland D, Voelker DR. Phosphatidylglycerol suppresses influenza A virus infection. Am J Respir Cell Mol Biol. 2012;46:479–487. [PMC free article] [PubMed]
29. Hallman M, Merritt TA, Bry K. The fate of exogenous surfactant in neonates with respiratory distress syndrome. Clin Pharmacokinet. 1994;26(3):215–232. [PubMed]
30. Shih AY, Denisov IG, Phillips JC, Sligar SG, Schulten K. Molecular dynamics simulations of discoidal bilayers assembled from truncated human lipoproteins. Biophys J. 2005;88:548–556. [PubMed]

Articles from International Journal of Nanomedicine are provided here courtesy of Dove Press