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Lassa Fever Virus Peptides Predicted by Computational Analysis Induce Epitope-Specific Cytotoxic-T-Lymphocyte Responses in HLA-A2.1 Transgenic Mice

Agnieszka Boesen, Krishnan Sundar, and Richard Coico^*

Department of Microbiology and Immunology, City University of New York Medical School, New York, New York 10031

Received 30 March 2005/ Returned for modification 17 May 2005/ Accepted 16 June 2005

	ABSTRACT

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Lassa fever is a hemorrhagic disease caused by Lassa fever virus (LV). Although the precise host defense mechanism(s) that affords protection against LV is not completely understood, cellular immunity mediated by cytotoxic T lymphocytes (CTLs) plays a pivotal role in controlling viral replication and LV infection. To date, there have been no reports mapping major histocompatibility complex (MHC) class I-binding CTL epitopes for LV. Using computer-assisted algorithms, we identified five HLA-A2.1-binding peptides of LV glycoprotein (GP) and two peptides from LV nucleoprotein (NP). Synthesized peptides were examined for their ability to bind to MHC class I molecules using a flow cytometric assay that measures peptide stabilization of class I. Three of the LV-GP peptides tested (LLGTFTWTL, SLYKGVYEL, and YLISIFLHL) stabilized HLA-A2. The LV-NP peptides tested failed to stabilize this HLA-A2. We then investigated the ability of the HLA-A2-binding LV-GP peptides to generate peptide-specific CTLs in HLA-A2.1 transgenic mice. Functional assays used to confirm CTL activation included gamma interferon enzyme-linked immunospot (ELISPOT) assays and intracellular cytokine staining of CD8⁺ T cells from peptide-primed mice. CTL assays were also performed to verify the cytolytic activity of peptide-pulsed target cells. Each of the LV-GP peptides induced CTL responses in HLA-A2-transgenic mice. MHC class I tetramers prepared using one LV-GP peptide that showed the highest cytolytic index (LLGTFTWTL) confirmed that peptide-binding CD8⁺ T cells were present in pooled lymphocytes harvested from peptide-primed mice. These findings provide direct evidence for the existence of LV-derived GP epitopes that may be useful in the development of protective immunogens for this hemorrhagic virus.

	INTRODUCTION

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Among the emerging infectious diseases, viral hemorrhagic fever (VHF) represents a serious public health problem with recurrent outbreaks worldwide (16). In addition to infections occurring in areas of VHF endemicity and those imported from such areas to other parts of the world, a new concern has recently emerged due to weaponization of these pathogens for use as bioweapons. Four distinct families of viruses are known to have members that cause VHF, including Arenaviridae, Bunyaviridae, Filoviridae, and Flaviviridae. Among the Arenaviridae family of viruses, Lassa fever virus (LV) is a pathogen that causes high mortality rates in infected individuals. It is known to have been weaponized, and it is thus designated a category A agent by the Centers for Disease Control and Prevention (9). LV is endemic in rural Africa and has been estimated to cause 300,000 infections/year and several thousand deaths due to hemorrhagic fever (15). The fatality rate of hospitalized patients is about 17%, but in certain groups of patients, such as pregnant women, there is a >30% mortality rate, and fetal and neonatal deaths approach 88% (7, 20). The principal vector for LV transmission in humans is Mastomys natalensis, a ubiquitous and highly commensal rodent host. LV infection in rodents is persistent and asymptomatic. However, once infected with this virus, animals exhibit profuse urinary excretion of LV. The virus is transmitted from rodents to humans by contact with animal urine or feces or even blood that contains high virus titers. Transmission between humans has been reported as a result of exposure to blood, sexual contact, and breast-feeding (15). The incubation period of Lassa fever may last up to three weeks. Therefore, the virus may be imported to other regions of the world while infected individuals are asymptomatic or show early nonspecific signs of LV infection. So far, about 20 cases of imported Lassa fever have been reported worldwide (4).

The molecular mechanisms underlying the pathogenicity of LV are not clearly understood. Currently, there are no vaccines available for LV and the only effective therapy available for the treatment of VHF caused by LV is the antiviral drug ribavirin (9). However, ribavirin treatment has been shown to be effective only if it is administered early after infection (14).

Although the mechanism of protection against LV is not completely understood, cell-mediated immunity is believed to play a pivotal role in controlling LV infection and replication (7, 28, 29). Neutralizing antibodies specific for LV are of low titers or nonexistent in infected individuals (23). Moreover, treatment of LV-infected individuals using pooled immunoglobulin containing high titers of anti-LV antibodies is not always effective (14). This observation suggests that humoral immunity plays a minor role in controlling infections caused by LV. Fisher-Hoch et al. (7) have demonstrated the critical role of T-cell response in controlling virus replication and preventing the cascade of events that leads to death. Their data strongly implicate the primary role of cytotoxic T lymphocytes (CTLs) in conferring protection from infection with LV. To date, there have been no reports identifying candidate protective CTL epitopes for this hemorrhagic virus.

In the current study we identified three HLA-A2.1-restricted CTL epitopes present within the LV glycoprotein (GP). These peptides were initially predicted as candidate epitopes using computer-assisted algorithms. The immunogenic properties of these LV epitopes were then confirmed using HLA-A2.1 transgenic mice together with functional assays to measure specific immune parameters associated with CTL responses.

	MATERIALS AND METHODS

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Computational prediction of candidate CTL epitopes for LV. Two matrix-based prediction algorithms, BIMAS (http://bimas.dcrt.nih.gov/molbio/hla_bind/) and SYFPEITHI (http://www.syfpeithi.de/Scripts/MHCServer.dll/EpitopePrediction.htm) were used for the prediction of LV peptides binding to HLA-A2.1 (19, 21). The amino acid sequences of LV (Josiah strain) nucleoprotein (NP-569AA; NCBI accession no. NP_694869.1) and glycoprotein (GP-491AA; NCBI accession no. NP_694870.1), each encoded by the S segment of LV RNA, were individually tested using these algorithms. The total NP and GP sequences were parsed into peptides of nine amino acids in length, each overlapping by eight amino acids. The selected peptides were then screened for similarity to the human genome using the National Institutes of Health (NIH) BLAST server (http://www.ncbi.nlm.nih.gov/BLAST/). Peptides showing homology with regard to the human proteome were eliminated from further study.

Cell line and peptides. TAP-deficient T2 cells expressing HLA-A2 were obtained from American Type Culture Collection (Manassas, VA) and maintained in Iscove’s modified Dulbecco medium (Invitrogen, Grand Island, NY) supplemented with 20% fetal bovine serum (Atlanta Biologicals, Lawrenceville, GA) at 37°C with 5% CO₂. All peptides used in this study were synthesized commercially (Sigma-Genosys, Woodlands, TX) and were of >95% purity. Peptides were dissolved either in water or dimethyl sulfoxide (DMSO) and diluted to desired concentrations in phosphate-buffered saline (PBS).

Mice. Six- to eight-week-old C57BL/6J transgenic mice expressing HLA-A2.1 [C57BL/6-TgN (HLA-A2.1) 1Enge] were obtained from The Jackson Laboratory (Bar Harbor, ME). The animals were maintained in our animal facility under specific-pathogen-free conditions.

MHC stabilization assay. The ability of peptides to bind to HLA-A2.1 molecules was evaluated using a major histocompatibility complex (MHC) class I stabilization assay (18). Briefly, T2 cells were grown overnight at 37°C in Iscove’s modified Dulbecco medium supplemented with 20% fetal bovine serum (FBS). Cells were harvested and washed twice with serum-free AIM-V medium (Invitrogen) and then incubated (5 x 10⁵/250 µl) with 50 µM of individual peptides at 37°C for 18 h in AIM-V medium. Following incubation, cells were washed twice with staining buffer (PBS plus 3% FBS) and stained for 30 min at 4°C with the fluorescein isothiocyanate (FITC)-conjugated anti-HLA-A2.1 antibody (Pharmingen, San Diego, CA) at a concentration of 500 ng per reaction in 100 µl of staining buffer. Stained cells were washed twice with staining buffer and resuspended in PBS. HLA-A2.1 expression was measured flow cytometrically using a BD LSRII flow cytometer (BD Biosciences, Mountain View, CA) and the data were analyzed using FlowJo software (Tree Star, Ashland, OR). A test peptide capable of causing a 150% increase in MFI values over the no-peptide control was considered a "high binder." The peptide GILGFVFTL, a well-known HLA-A2.1 epitope derived from influenza matrix antigen (17), was used as a positive control. The peptide IAGNSAYEY, a known HLA-A2.1 non-binder, was used as a negative control (3).

Generation of CTLs in HLA-A2.1 transgenic mice. Eight-week-old HLA-A2.1 transgenic female mice were immunized with 100 µg of individual test peptides together with 140 µg of an HBV-derived helper epitope (128-140AA). The peptides were emulsified in SEPPIC adjuvant-Montanide ISA 70 (Seppic, France) at a ratio of 1:1 and injected subcutaneously. Mice were boosted once following initial immunization and the splenocytes and lymph node cells were harvested one week after boosting to assess CTL responses.

In vitro CTL stimulation. Single-cell suspensions were prepared by pooling splenocytes and draining lymph node cells of immunized mice. Red blood cells (RBCs) were lysed using ACK lysis buffer and the cells were used immediately for enzyme-linked immunospot (ELISPOT) and intracellular cytokine staining assays. Alternatively, cells were cultured for 5 days in RPMI medium with 10% FBS, 10 mM HEPES, and 50 µM 2-mercaptoethanol supplemented with 10% T-stim (Pharmingen) and pulsed with 10 µM of antigenic peptides. Nonadherent CTLs were harvested and used as effector cells in the CTL assay described below.

ELISPOT assay. Peptide-specific T cells were enumerated using ELISPOT assays (13). ELISPOT plates (Pharmingen) were coated overnight at 4°C with 5 µg/ml of monoclonal anti-mouse gamma interferon (IFN-) antibody. After blocking the wells for 2 h with RPMI medium supplemented with 10% FBS, 100 µl of cell suspension (2 x 10⁶/ml) with different peptide concentrations (0.01 µM to 100 µM) was added to each well. A positive control (5 µg/ml concanavalin [ConA]) and a no-peptide negative control were included in all assays. The plates were incubated overnight at 37°C, in a 5% CO₂ humidified incubator. Following incubation, the wells were washed twice with deionized water and three times with wash buffer (PBS plus 0.05% Tween 20). Biotinylated anti-mouse IFN- was added to each well at the concentration of 2 µg/ml and the plates were incubated for 2 h at room temperature. After three washes, streptavidin-horseradish peroxidase (HRP) was added to each well and the plates were incubated for 1 h at room temperature. The plates were washed three times and colorimetric reactions developed using 3-amino 9-ethylcarbazole (AEC) substrate. ELISPOT assays were enumerated using a dissecting microscope, and values were expressed after subtracting the background.

Intracellular IFN- staining. Peptide-specific T cells were also measured by flow cytometric assessment of the IFN--containing T-cell phenotype as described previously (8). Intracellular IFN- production in pooled splenocytes and lymph node cells from immunized mice was measured following in vitro stimulation of cells with 1 µM (each) appropriate peptides. As a positive control, cells were also cultured overnight at 37°C in complete Iscove’s modified Dulbecco medium containing 20 ng/ml phorbol myristate acetate (PMA) and 1 µM ionomycin. Cultures of cells with no added peptides were used as negative controls. After incubation, 1 µl/ml of monensin (Golgi Stop; Pharmingen) was added to inhibit intracellular protein transport, and the cells were incubated for another 6 h. The cells were then washed and stained with monoclonal anti-CD8 PerCP (Pharmingen) in 1% FBS-PBS. The cells were then permeabilized with a Cyofix/Cytoperm kit (Pharmingen) and stained with FITC-conjugated monoclonal anti-IFN-. Cells were then analyzed flow cytometrically with a FACS LSR II analyzer and the number of IFN--containing CD8 cells was enumerated using FlowJo software.

CTL assay. CTL assays were performed using a nonradioactive CTL assay kit, CytoTox96 (Promega, Madison, WI), that measures lactate dehydrogenase (LDH) released by target cells in accordance with manufacturer’s instructions. T2 cells were used as target cells and were pulsed overnight with individual test peptides (10 µM). Peptide-stimulated effector cells from immunized mice were incubated with these peptide-loaded T2 target cells at different effector/target cell ratios ranging from 40:1 to 5:1 in a 96-well U-bottom plate for 4 h at 37°C. Fifty microliters of culture supernatants was then harvested from each well and tested for LDH activity using a chromogenic substrate. Absorbance was measured at 495 nm using an enzyme-linked immunosorbent assay (ELISA) reader (Bio-Rad, Hercules, CA). The percent specific cell lysis was calculated using the following formula: 100 x [(experimental - effector spontaneous) – target spontaneous]/[target maximum - target spontaneous].

Tetramer staining. Tetramer staining was performed as described by Singh et al. (26). HLA-A2.1-peptide tetramers were prepared by the NIAID Tetramer facility (Emory University, Atlanta, GA [http://emory.edu/WHSC/TETRAMER/]). Briefly, splenocytes from peptide-immunized and nonimmunized mice were harvested, RBCs lysed, and cells cultured overnight with the appropriate peptide (or no peptide) and then prepared for tetramer staining. One million cells (in 100 µl PBS containing 2% FBS and 0.02% sodium azide) were first stained with phycoerythrin (PE)-conjugated HLA-A2.1-peptide tetramers (1:800 dilution) for 30 min at room temperature, and then with a cocktail of PerCP-conjugated anti-CD3 and anti-CD8-FITC monoclonal antibodies (100 ng each) for 30 min at 4°C in the dark. The cells were washed twice and analyzed by fluorescence-activated cell sorter (FACS).

	RESULTS

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Computational prediction of CTL epitopes. The total protein sequences of LV-NP or LV-GP were parsed into peptides of nine amino acids in length, each overlapping by eight amino acids, as described in Materials and Methods. The ten highest-ranking peptides for GP and NP analyzed by BIMAS and SYFPEITHI are shown in Table 1.

Evaluation of synthetic peptides as candidate CTL epitopes. When evaluated for MHC class I binding, three out of the five selected GP-derived peptides (LLG, YLI, and SLY) stabilized the expression of HLA-A2.1 on T2 cells, as evidenced by their MFI profiles when compared with the no-peptide control (Fig. 1). An increase in MFI values of >300% was noted with the LLG and SLY peptides. This increase was similar to that observed using the positive peptide GIL. The YLI peptide caused a 175% increase in MFI over the no-peptide control (Table 2). The other two GP peptides, GLV and WLV, induced 60% and 0% increases in MFI, respectively. Thus, based on our selection criterion for the identification of peptides as high binders, nanomers LLG, SLY, and YLI were selected as candidates among the LV-GP peptides for further analysis. Neither of the computationally selected NP-derived LV peptides (CML and GILK) was able to stabilize HLA-A2.1 expression on T2 cells (Fig. 1; Table 2). Thus, these peptides were excluded as candidates for further study.

View larger version (21K): [in this window] [in a new window]   FIG. 1. Peptide binding to HLA-A2 as assessed by MHC class I stabilization. The ability of peptides to stabilize HLA-A2 on the surface of T2 cells was assessed by flow cytometric analysis after staining peptide-treated cells with anti-HLA-A.2 antibody. A positive control peptide, GILGFVFTL (GIL), was tested along with LV-GP peptides LLGTFTWTL (LLG), WLVSNGSYL (WLV), GLVGLVTFL (GLV), SLYKGVYEL (SLY), and YLISIFLHL (YLI), and LV-NP peptides CMLDGGNML (CML) and GILKSILKV (GILK). Each peptide was used at a 50 µM concentration. A positive shift (to the right) at varying degrees was observed with all the peptides except WLV, where a negative shift (to the left) was observed.

IFN- ELISPOT assay. Peptide-specific T cells were enumerated by measuring IFN--producing cells by ELISPOT assay. As shown in Fig. 2, a substantial number of T cells harvested from mice immunized with peptides responded by producing IFN-. We observed a dose-dependent relationship between the concentration of peptide used for stimulation and the IFN--producing T cells (Fig. 2). Two of the LV-GP peptides, LLG and SLY, were found to be more effective in generating peptide-specific T cells by virtue of their ability to produce IFN- than the other high-binder peptide, YLI. The frequency of IFN--producing cells in the LLG- and SLY-primed splenocyte population was found to be 225 and 235 per one million cells, respectively, when cells were stimulated with 100 µM peptide (Fig. 2). These results were similar to those observed using the positive control GIL peptide (255 per million cells). The frequency of IFN--producing cells generated in response to YLI (100 µM) was 155/10⁶ cells. Similar to results observed with each of the other peptides tested, this response decreased with decreasing peptide concentrations, showing a dose-dependent profile. Interestingly, the nonbinding peptide, WLV, failed to either prime or to stimulate splenocytes from WLV-primed mice for IFN- production (Fig. 2).

View larger version (20K): [in this window] [in a new window]   FIG. 2. Enumeration of IFN--producing cells by ELISPOT. The IFN- ELISPOT assay was performed as described in Materials and Methods. LV-GP-derived peptides tested included LLG, WLV, SLY, and YLI (abbreviations for nanomer peptides are given in the legend of Fig. 1). A peptide (GIL) derived from influenza matrix antigen was used as a positive control. Peptide-specific ELISPOT assays reflect total number of spots minus backgrounds observed in the absence of peptide. The experiment was performed at least three times and the results shown represent the mean IFN- ELISPOTs/106 ± the standard deviation from a representative experiment.

Intracellular IFN- staining.

View larger version (46K): [in this window] [in a new window]   FIG. 3. Enumeration of CD8-positive IFN--producing cells by ICCS. Splenocytes and lymph node cells were pooled from peptide-immunized mice (n = 3 per peptide tested) and then stimulated in vitro with 10 µM of corresponding peptides and stained with CD8- and IFN--specific antibodies. Abbreviations for nanomer peptides are given in the legend of Fig. 1. The left panels indicate results of peptide-stimulated cells; the right panels indicate results of corresponding unstimulated controls.

View larger version (19K): [in this window] [in a new window]   FIG. 4. CTL responses by peptide-primed effector cells from HLA-A2.1 transgenic mice. Peptide-pulsed T2 cells were cocultured with pooled splenocytes and lymph node cells from corresponding peptide-primed HLA-A2.1 transgenic mice (n = 3 per peptide tested). LV-GP peptides tested included LLG, SLY, YLI, and a positive control peptide (GIL) derived from influenza matrix antigen (abbreviations for nanomer peptides are given in the legend of Fig. 1). Immune effector cells were incubated with target cells at the effector/target ratios shown. CTL assays were performed following a 4-h incubation period. Data points represent the mean percent specific lysis ± the standard deviation as measured by quantitation of LDH release. Results from a representative experiment among three performed are shown.

View larger version (34K): [in this window] [in a new window]   FIG. 5. Enumeration of LV LLG-specific CTLs by tetramer staining. Tetramer-positive antigen-specific T lymphocytes were analyzed in spleen and draining lymph nodes from LLG peptide-immunized and nonimmunized control HLA-A2.1 transgenic mice. Prior to staining, LLG-primed cells were stimulated in vitro overnight with 10 µM of LLG peptide; control cells were cultured in the absence of peptide. Lymphocytes were stained with the LLG/HLA-A2.1-PE-conjugated tetramers (1:800), FITC-conjugated anti-CD3, and PerCP-conjugated anti-CD8 monoclonal antibodies.

	DISCUSSION

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Experimental strategies that utilize computational methods combined with in vitro/in vivo studies have proven to be very useful in the identification of immunogenic T-cell epitopes from defined antigens (10, 30). Using two matrix-based algorithms, BIMAS and SYFPEITHI, we were able to predict epitopes within the GP and NP structural proteins of LV. Using quantitative flow cytometric parameters as criteria to define candidate epitopes, we selected five peptides from LV-GP and two peptides from LV-NP as predicted MHC class I binders (Table 1). The utility of the BIMAS and SYFPEITHI algorithms in predicting viral and tumor antigen-specific CTL epitopes has been demonstrated by many other groups (10, 12, 27, 30, 31). Previous studies have also validated the use of computational algorithms by mapping CTL epitopes previously identified using conventional methods to explore immunogenic motifs of pathogens (25). Based on our computational prediction data, the following GP-derived peptides were selected for testing of MHC class I binding ability: LLGTFTWTL (LLG), WLVSNGSYL (WLV), GLVGLVTFL (GLV), and YLISIFLHL (YLI), SLYKGVYEL (SLY). We also investigated two selected NP-derived LV peptides: CMLDGGNML (CML) and GILKSILKV (GILK).

The glycoprotein precursor of LV-GP is posttranslationally cleaved into two proteins, GP1 and GP2. The epitopes SLY and YLI lie on GP1 and GP2, respectively. It is interesting to note that the peptide LLG lies right at the cleavage site that is between L259 and G260 (11). Since the cleavage is a post-translational modification, some of the precursor proteins produced may escape cleavage and be subjected to proteosomal digestion. Thus, we can't rule out the possibility of LLG presented as a CTL epitope. It would be interesting to see whether this is the case in human LV infections

To validate the ability of these predicted class I binders to ligate HLA-A2.1, we employed an MHC class I stabilization assay. Three out of the five selected GP-derived peptides (LLG, YLI, and SLY) stabilized the expression of HLA-A2 molecules expressed on T2 cells, as evidenced by a positive shift in MFI relative to the no-peptide control. T2 cells treated with the other two GP-derived peptides (WLV and GLV) did not show any appreciable increase in MFI when stained with FITC-conjugated anti-HLA-A2-specific monoclonal antibody. Indeed, the peptide WLV caused a negative shift in MFI (Fig. 1), suggesting destabilization of HLA-A2 expressed by T2 cells. Neither of the computationally selected NP-derived peptides (CML and GILK) stabilized HLA-A2 expression on these cells (Fig. 1; Table 2). Despite the fact that each of these nonstabilizing peptides contained the required anchoring amino acid residues (L, M, or I at the second position; V at the ninth position), they failed to bind HLA-A2 when evaluated using this class I stabilization assay. It has been shown that the success rate of these algorithms in predicting MHC class I binding ranges broadly from 30 to 70% depending on the class I allele and peptide motif under study (6, 24). Other factors that contribute to the success or failure of these prediction algorithms to map MHC class I-binding epitopes include peptide length, spacing between required anchoring residues, and the presence of other amino acids which may act as secondary anchor residues that may play a role in binding (5, 22, 32). Combinations of these factors may also influence the ability of peptides to bind MHC class I molecules. Thus, it is difficult to accurately explain the failure of some of the LV-derived peptides identified computationally as candidate epitopes to stabilize HLA-A2.1 molecules.

Peptide-induced stabilization of MHC class I molecules is directly correlated with their ability to induce CTL response in vivo (24). Based on the MHC class I binding profiles of the LV peptides tested, LLG, YLI, and SLY were selected for in vivo studies. As an LV peptide-negative control, the HLA-A2.1 nonbinding peptide WLV was included in initial ELISPOT studies to measure the ability of peptides to induce IFN--secreting cells. As shown in Results, the high-binding peptide LLG was found to induce stronger T-cell responses than the other LV-GP peptides tested. When we measured intracellular cytokine responses induced by these peptides, however, YLI was found to consistently induce higher levels of IFN- than LLG and SLY (Fig. 3). As expected, the HLA-A2.1 nonbinder (WLV) failed to induce T-cell responses as measured by IFN- ELISPOT assay.

ELISPOT quantitation of IFN--secreting cells yielded results that correlated well with CTL responses. T cells from LV peptide-primed HLA-A2.1 transgenic mice efficiently lysed corresponding LV peptide-loaded target cells. Among the LV peptides tested for their ability to generate peptide-specific CTLs, LLG induced the highest responses at the 40:1 E:T ratio, followed by SLY and YLI, respectively.

In light of the efficiency of LLG in generating CTL responses, we prepared LLG-HLA-A2.1 tetramers to allow us to perform more quantitative and confirmatory studies to enumerate LLG-specific cells flow cytometrically (1). Tetramer staining of pooled splenocytes and lymph node cells from LLG-primed mice confirmed the presence of a small but significant population (0.32%) of LLG-specific CD8⁺ T cells.

Given the biosafety issues associated with LV and the paucity of individuals previously exposed to this virus, our knowledge of protective immunity to this hemorrhagic virus is far from complete. Recently it has been shown that cellular immunity is clearly associated with recovery from a natural course of LV infection (28, 29). ter Meulen et al. (28) have examined CD4⁺ T cells with regard to their LV epitope specificity and identified six T helper epitopes (NP specific) using overlapping epitopes expressed within the NP structural protein. In a more recent study by these investigators (29), overlapping peptide pools as well as single peptides derived from LV-GP were screened to map CD4⁺ T-cell epitopes. Using T-cell clones generated from peripheral blood mononuclear cells (PBMC) obtained from LV-seropositive individuals, they identified three class II LV epitopes which were capable of inducing proliferative responses of PBMC. These epitopes were later confirmed using the prediction software, ProPred, indicating a good correlation between experimentally observed and computationally predicted HLA-DR-restricted peptides.

Heretofore, no other LV epitope mapping studies have been reported other than these two reports aimed at mapping MHC class II-binding motifs. Using nonhuman primates, another study demonstrated protection against live-virus challenge in animals vaccinated with glycoproteins GP1 and GP2 despite minimal LV-specific antibody responses, suggesting a greater role for T cell-mediated immunity (7).

A full understanding of the protective contribution of T-helper and CTL responses to LV together with broader knowledge of the immunogenic viral motifs that effectively induce such responses is not only of theoretical significance, but also of practical significance in designing appropriate vaccination strategies. Our approach to mapping and testing selected human MHC class I allele-specific LV binding motifs has confirmed the existence of three epitopes capable of generating peptide-specific CTL responses. The present study indicates that LV-GP peptides LLG and SLY are highly immunogenic and that YLI is moderately immunogenic in HLA-A2 transgenic mice. This is the first report describing MHC class I-binding CTL epitopes for LV. Future studies using nonhuman primates to examine these candidate immunogenic epitopes should be undertaken to confirm their ability to stimulate LV-specific effector T cells capable of protecting animals from challenge with live virus. Future studies to explore the utility of these mapped LV epitopes as diagnostic tools in monitoring and assessing T-cell immunity to this virus following infection or vaccination will also be useful.

	ACKNOWLEDGMENTS

 
We acknowledge the technical assistance of Viera Lima and Igor Toporovsky. We are also grateful to Jeffery Walker for his help with the flow cytometric analyses and Stephen O'Neill of SEPPIC Inc. for providing the adjuvant used in this work.

	FOOTNOTES

 
* Corresponding author. Mailing address: Department of Microbiology and Immunology, Weill Medical College of Cornell University, 1300 York Avenue, Room A128, New York, NY 10021. Phone: (607) 254-6554. Fax: (607) 254-6376. E-mail: ric2008{at}med.cornell.edu.

Present address: Allergic Inflammation Section, NIAID/NIH, Rockville, MD 20852.

Present address: Department of Medicine, UMDNJ—New Jersey Medical School, Newark, NJ 07103.

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