Survey
* Your assessment is very important for improving the workof artificial intelligence, which forms the content of this project
* Your assessment is very important for improving the workof artificial intelligence, which forms the content of this project
MAJOR ARTICLE Fluorescent Antigen–Transfected Target Cell Cytotoxic T Lymphocyte Assay for Ex Vivo Detection of Antigen-Specific Cell-Mediated Cytotoxicity Carel A. van Baalen, David Kwa, Esther J. Verschuren, Mariska L. Reedijk, Adrianus C. M. Boon, Gerrie de Mutsert, Guus F. Rimmelzwaan, Albert D. M. E. Osterhaus, and Rob A. Gruters Department of Virology, Erasmus MC, University Medical Center and Postgraduate School of Molecular Medicine, Rotterdam, The Netherlands Ex vivo detection of virus-specific cytotoxic T lymphocyte (CTL) responses is limited to the use of methods assessing cytokine production, degranulation, or perforin contents of antigen-specific CD8+ T cells. Generally, their cytotoxic activity is detectable only after cultivation. We describe the fluorescent antigen–transfected target cell–CTL (FATT-CTL) assay, which measures antigen-specific cytotoxicity ex vivo. Target cells were generated by nucleofection with DNA vectors encoding antigen–green fluorescent protein (GFP) fusion proteins. After coculture at various effector:target (E:T) cell ratios, viable and dead GFP-positive cells were quantified by flow cytometry, and antigen-specific target-cell elimination was calculated. The assay was validated with human immunodeficiency virus (HIV)– and influenza virus–specific CTL clones and revealed cytotoxicity at lower E:T cell ratios than standard 51Cr-release assays. Moreover, antigen-specific cytotoxicity was detected ex vivo within 1 day in peripheral blood mononuclear cells from HIV-infected individuals. The FATT-CTL assay provides a versatile tool that will advance our understanding of cell-mediated immunity. Virus-specific cytotoxic T lymphocytes (CTLs) contribute to the control of virus infection by eliminating infected cells and by producing antiviral cytokines [1]. During past decades, the most widely used method to study CTL-mediated cytotoxicity has been the 51Cr-release assay [2]. Recently, alternative methods for the detection of CTL responses have been developed, including enzyme-linked immunospot, intracellular cytokine staining (ICS), CD107 staining, and specific T Received 2 February 2005; accepted 13 May 2005; electronically published 30 August 2005. Presented in part: AIDS Vaccine 2004 International Conference, Lausanne, Switzerland, 30 August–1 September 2005 (abstract P166); HIV Vaccines: Current Challenges and Future Prospects, Keystone Symposia, Banff, Alberta, Canada, 9– 15 April 2005 (abstract 431); World Health Organization Consultation on Immunologic Assays to Evaluate Efficacy of Influenza Vaccines, Geneva, Switzerland, 25 January 2005. Potential conflicts of interest: none reported. Patent application on the technology is pending (Erasmus MC will be the patent owner). Financial support: Novaflu; European Union (grant QLRT-01034). R.A.G. is on sabbatical leave from the Centre National de la Recherche Scientifique. Reprints or correspondence: Dr. A.D.M.E. Osterhaus, Dept. of Virology, Erasmus MC, PO Box 1738, 3000 DR Rotterdam, The Netherlands ([email protected]). The Journal of Infectious Diseases 2005; 192:1183–90 2005 by the Infectious Diseases Society of America. All rights reserved. 0022-1899/2005/19207-0009$15.00 cell receptor staining by use of fluorescent major histocompatibility class (MHC) I peptide complexes [3– 6]. These methods are aimed at the detection of virusspecific CTLs in lymphocyte populations and do not directly measure the outcome of the full cytolytic cascade [7, 8]. Several nonradioactive alternatives for the 51 Cr assay have been developed for the study of the cytolytic activity of CTLs. These assays use fluorescent dyes to discriminate target and effector cells and to assess target-cell elimination [9–11]. When the epitopes are known, target cells can be sensitized for lysis by specific CTLs by pulsing them with excess peptide representing the epitope. For the detection of CTLs against unknown epitopes, sets of overlapping peptides spanning whole proteins can be used [12, 13]. A disadvantage of this approach is that, in addition to the costs related to peptide synthesis, the repertoire of epitopes recognized after the infection of cells may differ from that identified by exogenously added peptides [14, 15]. Moreover, differences in avidity and the protective potential of CTLs cannot be determined [16–18]. To achieve the endogenous processing of proteins, recombinant viral vectors like recombinant vaccinia virus are used for the infection Ex Vivo Cell-Mediated Cytotoxicity • JID 2005:192 (1 October) • 1183 Figure 1. Construction of plasmid DNA vectors for the expression of antigen–fluorescent protein fusion proteins. A, Construct of HIV genes encoding Rev, Tat, Gag, and Nef in the codon-optimized subtype B consensus sequence. B, Multiple cloning site of N1 Living Colors vectors. C, Spacer for creating an in-frame cloning site for the influenza virus genes. D, Influenza virus genes encoding nucleoprotein (NP) strain A/NL/18/94 (NP01), NP strain A/HK/2/ 68 (NP02), NP strain A/PR/8/34 (NP03), and matrix protein 1 (M1) strain A/NL/18/94. E, Expression of HIV-1 Rev–green fluorescent protein (GFP), Tat-GFP, and influenza virus NP01-GFP in nucleofected B lymphoblastoid cells. Left, Live-gated (FSC/TP3) B157 cells, 20 h after nucleofection with 5 mg pRev-GFP (solid lines, 53.3% in M1) or pTat-GFP (dashed lines, 59.4%) and with untreated B157 cells (dotted lines, 0.71%). Right, Live-gated (FSC/TP3) B3180 cells, 20 h after nucleofection with 4 mg of pNP01-GFP (solid lines, 30.7%) and untreated B3180 cells (dotted lines, 0.9%). of target cells [19]. In human studies, this use is complicated by the existence of preexisting immunity against the vector, which often results in high levels of background CTL immunity at baseline. Direct expression of the relevant protein antigens from plasmid DNA in appropriate MHC-matched target cells would circumvent this problem [3]. However, classic transfection techniques usually result in poor viability, as well as in low transfection efficiencies, and long-term cultures of cells in selective media are required to obtain sufficient numbers of antigen-presenting cells (APCs). For the development of a versatile, nonradioactive procedure to measure T cell–mediated cytotoxicity, we used nucleofection, a novel transfection technology that enables the rapid and highlevel expression of foreign genes in resting and activated cells [20, 21]. In this assay, fluorescent antigen–transfected target cells (FATT) are cocultured with CTL effector cells, and their killing by CTLs is monitored by flow cytometry. MATERIALS AND METHODS Effector cell lines and clones. The generation and culture of the CD8+ T cell clones used in the present study have been de1184 • JID 2005:192 (1 October) • van Baalen et al. scribed elsewhere [22–24]. The clones were 709TCC108, which is specific for the HIV Rev67–75 epitope SAEPVPLQL; TCC-C10, the influenza A nucleoprotein (NP)418–426 epitope LPFEKSTVM, which is restricted via HLA-B*3501; TCC3180, the influenza A NP418–426 epitope LPFEKSTVM, which is restricted via HLAB*3501; TCC1.7, the influenza A NP44–52 epitope CTELKLSDY, which is restricted via HLA-A*0101; and TCCM1/A2, the influenza A matrix protein 1 (M1)58–66 epitope GILGFVFTL, which is restricted via HL-A*0201. The cells were cultured for at least 7 days after stimulation with phytohemagglutinin (PHA) and feeder cells before their use as effector cells in CTL assays. Vectors. The cloning strategy for the construction of vectors plasmid (p) Rev–green fluorescent protein (GFP), pTatGFP, pGag-GFP, pNef-GFP, pNP01-GFP, pNP02-GFP, pNP03GFP, and pM1-GFP is depicted in figure 1. Genes were cloned into the multiple cloning site of the Living Colors vector pEGFP-N1 (BD Biosciences) in frame with the fluorescent protein open-reading frame (ORF) by use of the indicated restriction enzymes. By omitting the stop codon of the cloned genes, a read through of the fluorescent gene was achieved. HIV genes were codon-optimized consensus subtype B synthetic genes (GeneArt). Influenza virus genes were derived from NP strain A/NL/18/94 (NP01), NP strain A/HK/2/68 (NP02), NP strain A/PR/8/34 (NP03), and M1 strain A/NL/18/94 (M1) [25, 26]. Inserts were sequenced completely, to confirm that no errors had been introduced and that they were expressed in frame with the fluorescent protein ORF. Sequences have been submitted to GenBank (accession numbers AY936877–AY936886). Plasmid DNA was prepared by use of the Endo-Free Plasmid maxi kit from Qiagen, in accordance with the manufacturer’s instructions. Vector DNA prepared with this kit contains !0.1 endotoxin units (0.046 ng of lipopolysaccharide)/mg of DNA (see http://www1.qiagen.com for further details). Target cells. Two Epstein-Barr virus (EBV)–transformed B lymphoblastoid cell lines (BLCLs), B157 and B3180, were used as sources of autologous or HLA-matched target cells for the CTL clones. BLCLs were cultured in RPMI 1640 supplemented with 2 mmol/L l-glutamine, 100 U/mL penicillin, 100 mg/mL streptomycin, 1 ⫻ 10⫺5 mol/L 2-mercaptoethanol, and 10% fetal bovine serum (R10F; Greiner, Bio-One). Antigen expression was achieved by transfecting BLCLs with plasmid DNA vectors by use of the Amaxa Nucleofector technology, in accordance with the manufacturers’ instructions. Briefly, 1–2 ⫻ 10 6 cells in the logarithmic growth phase were resuspended in 100 mL of nucleofection buffer (Amaxa) that contained 2–4 mg of DNA; they were then subjected to one of the electroporation programs. Subsequently, cells were cultured overnight in a final volume of 2–4 mL of R10F in 5% CO2 at 37C. All buffers and programs of the Cell Line Optimization Nucleofector kit (Amaxa) were tested, and the combination of buffer V with program P-16 (Amaxa) resulted in the highest concentration of viable GFP-expressing cells, combined with high overall viability—that is, 50% after 24 h (data not shown). Target cells for the ex vivo FATT-CTL assay were generated by nucleofecting freshly isolated peripheral blood mononuclear cells (PBMCs) by use of the optimized Human T Cell Nucleofector kit (Amaxa), as described below. This resulted in 30%–70% GFP-positive events in live-gated populations after 24 h. FATT-CTL assay (4 h). Target cells were washed and cocultured with effector cells at increasing effector:target cell (E:T) ratios in 200 mL of R10F in 5% CO2 for 3–4 h at 37C. Cells were transferred to wells or tubes that contained 5 mL of EDTA (final concentration, 2.5 mmol/L), to reduce the number of cell-cell conjugates, and 5 mL of TO-PRO-3 iodide (TP3; final concentration, 25 nmol/L; Molecular Probes), to discriminate between viable and nonviable cells [10]. In some experiments, EDTA/TP3-treated cells were cooled on ice and stained with anti–CD8–phycoerythrin (PE; BD Biosciences) for 20 min before acquisition. The 51Cr-release assay was performed as described elsewhere [22]. Samples were acquired on a FACSCalibur device (BD Biosciences) for a fixed period of 60 s/sample. The forward scatter (FSC) acquisition threshold was set to include nonviable events. Debris was excluded by gating in FSC- TP3 dot plots during data analyses. The flow rate was plotted in a time-event histogram and generally proved to be constant in each of the samples per experiment. If it was not, we defined a region to select a shared period of constant flow rate. A region to exclude GFP-negative events was defined in GFP-TP3 or GFP-FL3 dot plots of the data acquired from cultures that contained BLCLs that had not been nucleofected. GFP-positive events derived from cultures that contained nucleofected BLCLs were displayed in FSC-TP3 or GFP-TP3 dot plots for the definition of viable GFP-positive (VG) events—that is, TP3-negative events—and nonviable or dead GFP-positive (DG) events— that is, TP3-positive events (figure 2A). Percentages of dead GFP-positive events (%DG) were calculated with the formula 100 ⫻ (number of DG)/(number of VG + number of DG). CTLmediated target-cell elimination was calculated with the for- Figure 2. Antigen-specific killing of fluorescent antigen–transfected B lymphoblastoid cells and peripheral blood mononuclear cells (PBMCs) by cloned cytotoxic T lymphocyte (CTL) populations. A, Green fluorescent protein (GFP)– and TP3-fluorescence intensities of pRev-GFP– (top) or pTat-GFP– nucleofected (bottom) B157 cells that had been cocultured with or without cells of a Rev-specific CTL clone at the indicated effector:target (E:T) ratios for 4 h. The mean fluorescence intensity of control GFP-negative events was ∼4. Nos. of viable and dead GFP-positive events detected during a fixed acquisition period of constant flow rate are indicated. The percentage of dead GFP-positive events is shown in parentheses. B, left, Percentage CTL-mediated lysis with values as shown in panel A. Initial E:T ratios were calculated from nos. of CD8+ and GFP-positive events detected in cultures that contained effector or target cells only, at 0 h. B, right, Antigen-specific lysis of pNP01-GFP–nucleofected PBMCs by cells of the influenza virus nucleoprotein (NP)–specific CTL clone TCC-C10. Ex Vivo Cell-Mediated Cytotoxicity • JID 2005:192 (1 October) • 1185 Figure 3. Comparison between 51Cr-release and fluorescent antigen– transfected target cell–cytotoxic T lymphocyte (FATT-CTL) assays. B157 cells were nucleofected with pRev–green fluorescent protein (GFP) or pTat-GFP; after overnight incubation, one-half of the cells were labeled with 51Cr and used as target cells in a standard 4-h 51Cr-release assay. The other half was tested in a 4-h FATT-CTL assay. Target cells were cocultured with Revspecific CTLs at indicated effector:target (E:T) ratios, and percentages of specific lysis were determined as described in Materials and Methods. T*, calculation of the initial E:T ratio in the FATT-CTL assay including GFPpositive and GFP-negative target cells, to allow a direct comparison between the 2 assays. mula 100 ⫻ (%DG+E ⫺ %DG⫺E )/(100 ⫺ %DG⫺E ), where +E and ⫺E denote the presence and absence, respectively, of effector cells in the cultures. Ex vivo FATT-CTL assay (18–24 h). PBMCs were isolated by density centrifugation (Lymphoprep; Nycomed) of heparinized blood (28–30 mL) obtained from 4 HIV-1–seropositive individuals attending the Erasmus MC who had received no antiretroviral therapy, had CD4 counts of 1300 cells/mm3, and had a viral load between 50 and 1 ⫻ 10 5 RNA copies/mL. Informed consent was obtained from all patients. We isolated PBMCs from buffy coats obtained from healthy blood donors as controls. Freshly isolated PBMCs (2 ⫻ 10 6 cells/cuvette) were nucleofected with plasmid DNA vectors (2 mg) by use of the Human T Cell Nucleofector kit (Amaxa), in accordance with the manufacturer’s instructions, and incubated in a humidified incubator in 1.5– 2.0 mL of R10F in 5% CO2 at 37C. Four hours later, a 50-mL sample was diluted 4-fold in R10F and acquired for 60 s for the determination of the number of GFPpositive events per time unit. The volume per time unit (flow rate) was determined in parallel for each experiment by use of tubes that contained a calibrated number of beads (TruCOUNT tubes; BD Biosciences) and 2 mL of FACSFlow sheath fluid (BD Biosciences), without antibodies. The concentration of viable GFP-positive events was generally between 1 ⫻ 10 5 and 3 ⫻ 105 cells/1.6 mL. Between 3 ⫻ 10 3 and 5 ⫻ 10 3 GFP-positive events were seeded per well and were cocultured with or without untreated PBMCs at a PBMC:GFP-positive cell ratio of ∼150 (triplicates) in conical 96-microwell Thermo-Fast 96 de1186 • JID 2005:192 (1 October) • van Baalen et al. tection plates (ABgene), in a total volume of 200 mL/well with or without recombinant interleukin (rIL)–2 (50 IU/mL). After overnight incubation, the cultures were transferred to 1.4mL U-tubes (Micronic) that contained 5 mL of EDTA (final concentration, 2.5 mmol/L) and 5 mL of TP3 (final concentration, 25 nmol/L), incubated for 20 min at 37C, transferred to melting ice, and acquired on a FACSCalibur within 2 h. To prevent event count rates being 12000 total events/s, we set an FL1 threshold during acquisition to exclude the majority of GFP-negative events, in addition to an FSC threshold to exclude debris. Because many killed GFP-positive cells can no longer be detected as TP3 positive, for GFP-positive events after an overnight incubation period (data not shown), we used the difference between the number of VG events in cultures with (VG+E) and without (VG⫺E) effector PBMCs to calculate the percentage of PBMC-mediated antigen-specific target-cell elimination: 100 ⫻ (VG⫺E ⫺ VG+E )/VG⫺E. ICS. ICS was performed with the BD FastImmune CD8 cytokine 4-color kit (BD Biosciences), in accordance with the manufacturer’s instructions. Overlapping peptide sets spanning Gag or Nef (15-mers with 11 overlap, HXB2; National Institutes of Health AIDS Research and Reference Reagent Program) were added to 1 mL of whole blood each (final concentration, 4 mg/ mL for each peptide) and incubated for 6 h in the presence of a CD28/CD49d monoclonal antibody mixture and brefeldin A (both of which were included in the kit). Unstimulated (1 mL) and staphylococcal enterotoxin B–stimulated (1 mg/mL; Sigma) blood samples were included as negative and positive controls, respectively. After the lyse/fix and permeabilization steps, cells were stained with CD8 peridinin-chlorophyll-protein complex– Cy5.5/CD3 allophycocyanin and anti–human interferon (IFN)– g fluorescein isothiocyanate/CD69 PE or isotype controls, ac- Figure 4. Cytotoxic T lymphocyte (CTL)–mediated killing of target cells expressing recombinant influenza virus nucleoprotein (NP)— or matrix protein 1 (M1)–green fluorescent protein (GFP). B3180 cells were nucleofected with pNP01-GFP, pNP02-GFP, pNP03-GFP, or pM1-GFP. The next day, these cells were cocultured for 3 h with or without TCC1.7, TCC-C10, TCC3180, and TCCM1/A2 cells at CD8+ :GFP-positive cell ratios of 10, 10, 5, and 2, respectively. CTL-mediated target-cell elimination was determined as described in Materials and Methods. Table 1. Specific lysis of nucleoprotein (NP)–green fluorescent protein–positive cells by different CD8+ T cell clones. CD8+ T cell clone Gene Epitope NP01/02/03 NP01 NP02 NP03 M1 NOTE. CTELKLSDY LPFEKSTVM ---D-P-I---DRT-IGILGFVFTL TCC1.7 TCC-C10 TCC3180 TCCM1/A2 a 50 … … … … … … 0.8 0.5 15 ⫻ 103 26 1104 1100 … … … … … … 50 M1, matrix protein 1. a Functional avidity: EC50 (nanomolar) of the cytotoxic T lymphocyte clones for the epitope variants, as determined in a 51Cr-release assay [24]. quired on a FACSCalibur, and analyzed by use of CellQuest software (version 4.0.2; BD Biosciences). RESULTS CTL-mediated lysis of fluorescent antigen–transfected BLCLs and PBMCs. Genes encoding viral proteins of HIV (rev and tat) and influenza A virus (nucleo- and matrix-protein) were inserted in frame with GFP in the pEGFP-N1 plasmid, as depicted in figure 1. Nucleofection of cells of the EBV-transformed lymphoblastoid cell line (BLCL) B157 with pRev-GFP and pTat-GFP resulted in 50%–60% GFP-positive cells (figure 1E). Antigen processing and the presentation of antigen-fluorescent fusion proteins (Ag-FP) was first assessed by coculturing pRev-GFP–transfected B157 cells with cells of the Rev-specific CTL clone (709TCC108) at increasing E:T ratios. We used pTatGFP–transfected B157 cells as negative controls. After 4 h of incubation, percentages of dead target cells—that is, TP3-positive, GFP-positive cells—increased from 20% to 84% in an E: T ratio–dependent fashion. The proportion of nonviable control target cells did not increase (figure 2A). After we corrected the values for spontaneous background dead cells, the antigenspecific cytolytic activity of the Rev-specific CTLs at E:T ratios of ∼0.3, ∼1, and ∼3 were 18%, 58%, and 80%, respectively (figure 2B, left). Next, we explored the use of fresh PBMCs as target cells. The nucleofection efficiency of unstimulated PBMCs or CD8+ cell–depleted PBMCs was typically between 30% and 70% (data not shown), which proved to be sufficient for their use as target cells. MHC class I–matched PBMCs, nucleofected with pNP01-GFP, were lysed by the CTL clone TCC-C10 and thus could be used as target cells in the FATT-CTL assay (figure 2B, right). The FATT-CTL assay was compared with a standard 51Crrelease assay by use of the same target- and effector-cell populations in both assays. Again, 55%–60% viable GFP-positive events were detected among pRev-GFP– and pTat-GFP–transfected B157 cells. Under the assumption that CTL epitopes were generated in the GFP-positive cells only, this would be the maximum level of specific lysis that could be achieved in the 51Cr- release assay. Indeed, 58% specific lysis was observed at the highest E:T ratio, 10 (figure 3). When the FATT-CTL assay was used, 190% of the GFP-positive cells were lysed by Rev-specific CTLs after 4 h at the highest E:T ratio. Specific lysis of pTat-GFP– positive cells was !3% for all E:T ratios tested in both assays (data not shown). Overall, the FATT-CTL assay detected cytotoxicity at significantly lower E:T ratios than the 51Cr-release assay (figure 3). Part of the increased sensitivity is most likely due to the ability to discriminate between cells expressing the gene of interest from cells that do not. This was supported by the results of separate experiments with influenza A virus NP-GFP constructs and the NP-specific CTL clone TCC-C10. Maximal CTL-mediated 51Cr release never exceeded the fractions of NP-GFP–expressing target cells, which were ∼20% in these experiments (data not shown). Parallel flow-cytometric analyses confirmed that the number of effector cells added to these cultures was sufficient to eliminate 190% of the GFP-positive cells (data not shown). CTL assays with influenza A virus–specific CTLs and epitope variants. To study the effects of epitope variation on the outcome of the FATT-CTL assay, we generated expression vectors encoding various influenza A virus NP- and M1-GFP fusion proteins. Three vectors were generated from NP-genes derived from distinct influenza virus strains: pNP01-, pNP02-, and pNP03-GFP. These genes contained the same HLA-A*0101 epitope NP44–52 sequence but differed in the HLA-B*3501 epitope NP418–426 sequence (figure 4 and table 1). The pM1-GFP vector encoded the HLA-A*0201–restricted epitope M158–66. B3180 cells, which express HLA-A*0101, -A*0201, and -B*3501, were nucleofected with the different vectors (figure 1E) and were cocultured the following day for 3 h with or without cells of 3 different NP-specific CTL clones—TCC1.7, TCC-C10, and TCC3180—or the M1-specific CTL clone M1/A2. Between 60% and 70% specific lysis was detected among NP01-, NP02-, and NP03-GFP–positive cells in cultures that contained HLA-A*0101–restricted TCC1.7 CTLs specific for the conserved NP44–52 epitope (figure 4). HLA-B*3501–restricted TCC-C10 cells also specifically lysed NP01-GFP–positive cells (70%) but did not lyse NP02- and NP03-GFP– positive cells, in concordance with previously determined EC50 values of the corresponding peptide variants, ∼0.8, 15000, and 110,000 nmol/L, respectively [24]. NP01-GFP– positive cells were lysed with similar efficiency by TCC3180 cells that recognized the NP01 peptide variant, with an EC50 value of 0.5 nmol/L. The lower avidity of these cells for the NP02-variant peptide (EC50, 26 nmol/L) was reflected by an ∼4-fold lower level of specific lysis of NP02-GFP–positive cells, compared with NP01-GFP–positive cells (table 1). Cells expressing the NP03 variant (EC50, 1100 nmol/L) were not lysed by TCC3180. The M1-specific TCC-M1/A2 CTLs did Ex Vivo Cell-Mediated Cytotoxicity • JID 2005:192 (1 October) • 1187 Figure 5. Ex vivo antigen-specific peripheral blood mononuclear cell (PBMC)–mediated elimination of HIV-1 Gag–green fluorescent protein (GFP)– or Nef-GFP–expressing lymphocytes. PBMCs obtained from 4 HIV-1–seropositive individuals were nucleofected with pEGFP-N1, pGag-GFP, or pNefGFP after a 4-h coculture with autologous untreated PBMCs in the absence (individual RH1-021) or presence (individuals RH1-022, RH1-028, and RH1029) of 50 IU/mL recombinant interleukin–2 at PBMC:GFP-positive ratios of ∼150. After overnight incubation, viable GFP-positive cells were quantified by flow cytometry and used to calculate percentages of cell-mediated targetcell elimination. Values represent the average +SE of triplicates. Vertically arranged below the fluorescent antigen–transfected target cell–CTL (FATTCTL) assay results from individuals RH1-022, RH1-028, and RH1-029 are dot plots showing CD69 and interferon (IFN)–g expression of CD3+CD8+gated lymphocytes, 6 h after stimulation with no peptides or with HIV-1 Gag or Nef peptide pools. Nos. representing percentages of CD69+IFN-g– positive cells are indicated in each dot plot. not specifically lyse the NP-GFP–expressing cells but lysed 50% of M1-GFP–positive cells (table 1). Detecting antigen-specific cytotoxicity ex vivo. We tested whether the FATT-CTL assay could be applied to detect antigen-specific cell-mediated cytotoxicity directly ex vivo. To this end, PBMCs were obtained from 4 highly active antiretroviral therapy–naive HIV-seropositive individuals and 4 HIV-seronegative individuals. Some of the cells were used to generate target cells by nucleofection with pGag-GFP, pNef-GFP, or pEGFP-N1 as a control. Gag and Nef were chosen as antigens because they are among those most frequently recognized. Four hours later, nucleofected and autologous untreated 1188 • JID 2005:192 (1 October) • van Baalen et al. PBMCs were cocultured at PBMC:GFP-positive cell ratios of ∼150 with or without the addition of rIL-2. After overnight incubation, concentrations of viable GFP-positive events were used to calculate antigen-specific target-cell elimination. The specific elimination of Gag-GFP– and/or Nef-GFP–expressing cells, compared with that of GFP-expressing cells, was observed in the absence (individual RH1-021) or presence (individuals RH1-022, RH1-028, and RH1-029) of exogenous IL2 (figure 5). For individuals RH1-022, RH1-028, and RH1-029, no significant cytotoxicity was observed in the absence of IL2 (data not shown). Because of a limited number of cells, we could not determine cytotoxicity in the presence of IL-2 for individual RH1-021. No Gag- or Nef-specific cytotoxicity, compared with that of GFP alone, was observed for any of the 4 seronegative control subjects, irrespective of the presence of exogenous IL-2 (data not shown). These data illustrate the practical utility of the FATT-CTL assay to directly measure virus-specific CTL activity ex vivo. Next, we tested whether the PBMC-mediated elimination of target cells correlated with the presence of antigen-specific CD8+ T cells. To this end, we stimulated cells obtained from individuals RH1-022, RH1-028, and RH1-029 with pools of overlapping peptides spanning Gag or Nef and determined the percentages of CD3+CD8+ cells that responded by up-regulating CD69-expression and IFN-g production, using a standard ICS assay. Figure 5 shows that, when lysis was detected in the FATT-CTL assay, antigen-specific CD3+CD8+ cells were readily observed. DISCUSSION In the present article, a novel method for the measurement of CTL-mediated cytotoxicity, the FATT-CTL assay, has been described. This method is based on the use of target cells that have been transfected with plasmid DNA encoding the protein of interest as a fluorescent fusion protein. The procedure was evaluated with freshly isolated PBMCs and with HIV-1– and influenza virus–specific CTL clones, by use of autologous PBMCs or MHC class I–matched BLCLs as target cells. Compared with other methods for the measurement of CTL responses, the FATT-CTL assay offers a number of advantages. In contrast to the traditional 51Cr-release assay, it is performed without the use of radioactive isotopes. Target cells are discriminated from effector cells without the need to stain these cell populations with fluorescent dyes like PKH-26 or carboxyfluorescein diacetate succinimidyl ester [9–11]. The FATT-CTL assay facilitates the detection of CTL responses directed against entire proteins without the need for the generation of recombinant viral vectors or the use of sets of overlapping peptides. Potential high background CTL activity found against EBV and recombinant vectors, like vaccinia virus, which have been used in other assays to generate target cells expressing the antigen of choice, does not interfere with the outcome of the FATT-CTL assay. In contrast to the ex vivo detection of virus-specific CTLs with fluorescent oligomers of HLA class I peptide complexes or ICS of cytokines on the stimulation of CTLs with peptides representing known CTL epitopes, HLA typing of study individuals or the selection of common haplotypes is not required. The processing and presentation of endogenously expressed antigens mimic natural conditions more closely than does the use of exogenous synthetic peptides. In the experiments presented, HIV-1 subtype B genes were used, which may differ antigenetically from autologous viruses. Therefore, CTL responses to some epitopes may not have contributed to the elimination of target cells. Given the relative ease of generating new Ag-FP plasmids, analysis of the CTL repertoire against autologous variants and against rapidly changing epitopes and of the role that CTL-mediated immune pressure plays in individual patients is feasible. In vaccine trials, cell-mediated cytotoxicity can be assessed by use of Ag-FP plasmids that contain the vaccine antigen–encoding genes. The FATT-CTL assay with NP-specific TCC-C10 and TCC3180 cells reflected differences in their functional avidity for variant epitope sequences. TCC3180 cells killed autologous cells pulsed with saturating amounts of the LPFDKPTIM peptide (EC50, 26 nmol/L), but most of the cells expressing NP02, the NP variant containing the corresponding epitope sequence, were not killed. This could not be explained by limiting levels of NP expression in the target cells or the condition of the effector cells, as evinced by the killing of NP02-expressing cells by TCC1.7 cells or of NP01-expressing cells by TCC3180 cells, respectively. These data show that, according to the results of the FATT-CTL assay, differences in T cell–mediated cytotoxicity toward various epitope variants can be detected. Recent studies by other researchers have indicated that the use of saturating peptide concentrations may detect CTLs of low avidity that are unable to recognize tumor cells [27, 28]. Similar studies have been reported for the association between avidity and effective virus control [29, 30]. In HIV infection, virus control is associated with the induction and maintenance of antigen-specific CD8+ cells, especially if they express perforin [8, 31, 32], which indicates that their cytotoxic activity is an important effector mechanism. With the FATT-CTL assay, we can now directly assess the outcome of the cytolytic potential of CTLs, including those for which no fluorescent oligomers of HLA class I peptide complexes are available. For 3 of the 4 individuals that we studied, Gag- and Nef-specific cytotoxicity was found to be IL-2 dependent. The improvement of HIV-specific cytotoxicity by exogenous IL-2 has been reported to be associated with an increase in CD3z expression on CD8+ cells in HIV infection [33]. As for other ex vivo CTL detection methods, studies of the influence of costimulatory factors on ex vivo cytotoxicity can elucidate requirements for the optimal detection of cytotoxic T cell responses and of the mechanisms of T cell dysfunction in HIV infection [8]. In conclusion, the FATT-CTL assay offers unique opportunities for the specific and sensitive analysis of functional aspects of T cell–mediated cytotoxicity. This versatile method, with its practical and direct ex vivo format, will allow moreefficient studies of the role of CTL-mediated immunity as a correlate of protection in human and animal virus infections and in vaccine trials. Acknowledgments We acknowledge M. E. van der Ende (Department of Internal Medicine, Erasmus MC) and the individuals who donated blood, for their contribution to the study. The HIV-1 subtype B Gag and Nef (15-mer with 11 overlap, HXB2) peptides, complete set reagent was obtained through the AIDS Research and Reference Reagent Program, Division of AIDS, National Institute of Allergy and Infectious Diseases. References 1. Yang OO, Walker BD. CD8+ cells in human immunodeficiency virus type I pathogenesis: cytolytic and noncytolytic inhibition of viral replication. Adv Immunol 1997; 66:273–311. 2. Brunner KT, Mauel J, Cerottini JC, Chapuis B. Quantitative assay of the lytic action of immune lymphoid cells on 51-Cr-labelled allogeneic target cells in vitro: inhibition by isoantibody and by drugs. Immunology 1968; 14:181–96. 3. Sun Y, Iglesias E, Samri A, et al. A systematic comparison of methods to measure HIV-1 specific CD8 T cells. J Immunol Methods 2003; 272: 23–34. 4. Altman JD, Moss PA, Goulder PJ, et al. Phenotypic analysis of antigenspecific T lymphocytes. Science 1996; 274:94–6. 5. Rubio V, Stuge TB, Singh N, et al. Ex vivo identification, isolation and analysis of tumor-cytolytic T cells. Nat Med 2003; 9:1377–82. 6. Tomaru U, Yamano Y, Nagai M, et al. Detection of virus-specific T cells and CD8+ T-cell epitopes by acquisition of peptide-HLA-GFP complexes: analysis of T-cell phenotype and function in chronic viral infections. Nat Med 2003; 9:469–76. 7. Yang OO. Will we be able to “spot” an effective HIV-1 vaccine? Trends Immunol 2003; 24:67–72. 8. Lieberman J. Tracking the killers: how should we measure CD8 T cells in HIV infection? AIDS 2004; 18:1489–93. 9. Lecoeur H, Fevrier M, Garcia S, Riviere Y, Gougeon ML. A novel flow cytometric assay for quantitation and multiparametric characterization of cell-mediated cytotoxicity. J Immunol Methods 2001; 253:177–87. 10. Lee-MacAry AE, Ross EL, Davies D, et al. Development of a novel flow cytometric cell-mediated cytotoxicity assay using the fluorophores PKH26 and TO-PRO-3 iodide. J Immunol Methods 2001; 252:83–92. 11. Liu L, Chahroudi A, Silvestri G, et al. Visualization and quantification of T cell-mediated cytotoxicity using cell-permeable fluorogenic caspase substrates. Nat Med 2002; 8:185–9. 12. Maecker HT, Dunn HS, Suni MA, et al. Use of overlapping peptide mixtures as antigens for cytokine flow cytometry. J Immunol Methods 2001; 255:27–40. 13. Addo MM, Altfeld M, Rosenberg ES, et al. The HIV-1 regulatory proteins Tat and Rev are frequently targeted by cytotoxic T lymphocytes derived from HIV-1-infected individuals. Proc Natl Acad Sci USA 2001; 98:1781–6. 14. Hahn YS, Hahn CS, Braciale TJ. Endogenous presentation of a nascent antigenic epitope to CD8+ CTL is more efficient than exogenous presentation. Immunol Cell Biol 1996; 74:394–400. Ex Vivo Cell-Mediated Cytotoxicity • JID 2005:192 (1 October) • 1189 15. Schutten M, Van Baalen CA, Guillon C, et al. Macrophage tropism of HIV-1 facilitates in vivo escape from cytotoxic T lymphocytes. J Virol 2001; 75:2706–9. 16. Gallimore A, Hengartner H, Zinkernagel R. Hierarchies of antigenspecific cytotoxic T-cell responses. Immunol Rev 1998; 164:29–36. 17. O’Connor DH, Allen TM, Vogel TU, et al. Acute phase cytotoxic T lymphocyte escape is a hallmark of simian immunodeficiency virus infection. Nat Med 2002; 8:493–9. 18. Beattie T, Kaul R, Rostron T, et al. Screening for HIV-specific T-cell responses using overlapping 15-mer peptide pools or optimized epitopes. AIDS 2004; 18:1595–8. 19. Bennink JR, Yewdell JW, Smith GL, Moller C, Moss B. Recombinant vaccinia virus primes and stimulates influenza haemagglutinin-specific cytotoxic T cells. Nature 1984; 311:578–9. 20. Lai W, Chang CH, Farber DL. Gene transfection and expression in resting and activated murine CD4 T cell subsets. J Immunol Methods 2003; 282:93–102. 21. Maasho K, Marusina A, Reynolds NM, Coligan JE, Borrego F. Efficient gene transfer into the human natural killer cell line, NKL, using the Amaxa nucleofection system. J Immunol Methods 2004; 284:133–40. 22. Van Baalen CA, Schutten M, Huisman RC, Boers PH, Gruters RA, Osterhaus AD. Kinetics of antiviral activity by human immunodeficiency virus type 1-specific cytotoxic T lymphocytes (CTL) and rapid selection of CTL escape virus in vitro. J Virol 1998; 72:6851–7. 23. Boon AC, de Mutsert G, Fouchier RA, Sintnicolaas K, Osterhaus AD, Rimmelzwaan GF. Preferential HLA usage in the influenza virus-specific CTL response. J Immunol 2004; 172:4435–43. 24. Boon AC, de Mutsert G, van Baarle D, et al. Recognition of homoand heterosubtypic variants of influenza A viruses by human CD8+ T lymphocytes. J Immunol 2004; 172:2453–60. 25. Voeten JT, Rimmelzwaan GF, Nieuwkoop NJ, Fouchier RA, Osterhaus 1190 • JID 2005:192 (1 October) • van Baalen et al. 26. 27. 28. 29. 30. 31. 32. 33. AD. Antigen processing for MHC class I restricted presentation of exogenous influenza A virus nucleoprotein by B-lymphoblastoid cells. Clin Exp Immunol 2001; 125:423–31. Voeten JT, Rimmelzwaan GF, Nieuwkoop NJ, Lovgren-Bengtsson K, Osterhaus AD. Introduction of the haemagglutinin transmembrane region in the influenza virus matrix protein facilitates its incorporation into ISCOM and activation of specific CD8+ cytotoxic T lymphocytes. Vaccine 2000; 19:514–22. Zeh HJ III, Perry-Lalley D, Dudley ME, Rosenberg SA, Yang JC. High avidity CTLs for two self-antigens demonstrate superior in vitro and in vivo antitumor efficacy. J Immunol 1999; 162:989–94. Yee C, Savage PA, Lee PP, Davis MM, Greenberg PD. Isolation of high avidity melanoma-reactive CTL from heterogeneous populations using peptide-MHC tetramers. J Immunol 1999; 162:2227–34. Derby M, Alexander-Miller M, Tse R, Berzofsky J. High-avidity CTL exploit two complementary mechanisms to provide better protection against viral infection than low-avidity CTL. J Immunol 2001; 166: 1690–7. Gallimore A, Dumrese T, Hengartner H, Zinkernagel RM, Rammensee HG. Protective immunity does not correlate with the hierarchy of virus-specific cytotoxic T cell responses to naturally processed peptides. J Exp Med 1998; 187:1647–57. Migueles SA, Laborico AC, Shupert WL, et al. HIV-specific CD8+ T cell proliferation is coupled to perforin expression and is maintained in nonprogressors. Nat Immunol 2002; 3:1061–8. Lu W, Arraes LC, Ferreira WT, Andrieu JM. Therapeutic dendritic-cell vaccine for chronic HIV-1 infection. Nat Med 2004; 10:1359–65. Trimble LA, Lieberman J. Circulating CD8 T lymphocytes in human immunodeficiency virus-infected individuals have impaired function and downmodulate CD3 z, the signaling chain of the T-cell receptor complex. Blood 1998; 91:585–94.