Journal of Immunology Research

Journal of Immunology Research / 2013 / Article

Review Article | Open Access

Volume 2013 |Article ID 637649 |

Sandra A. Calarota, Fausto Baldanti, "Enumeration and Characterization of Human Memory T Cells by Enzyme-Linked Immunospot Assays", Journal of Immunology Research, vol. 2013, Article ID 637649, 8 pages, 2013.

Enumeration and Characterization of Human Memory T Cells by Enzyme-Linked Immunospot Assays

Academic Editor: Roslyn Kemp
Received06 Jun 2013
Accepted07 Sep 2013
Published11 Nov 2013


The enzyme-linked immunospot (ELISPOT) assay has advanced into a useful and widely applicable tool for the evaluation of T-cell responses in both humans and animal models of diseases and/or vaccine candidates. Using synthetic peptides (either individually or as overlapping peptide mixtures) or whole antigens, total lymphocyte or isolated T-cell subset responses can be assessed either after short-term stimulation (standard ELISPOT) or after their expansion during a 10-day culture (cultured ELISPOT). Both assays detect different antigen-specific immune responses allowing the analysis of effector memory T cells and central memory T cells. This paper describes the principle of ELISPOT assays and discusses their application in the evaluation of immune correlates of clinical interest with a focus on the vaccine field.

1. Introduction

The ELISPOT assay was originally developed to detect antigen-specific antibody-secreting B cells [1] and then evolved for the enumeration of antigen-specific cytokine-secreting T cells [2]. Since then the ELISPOT assay has been used to measure antigen-specific T cells by detecting cytokines secreted by T cells after stimulation with synthetic peptides (used as a pool or as single peptides) or whole antigens (such as proteins or lysates).

The ELISPOT assay not only permits the quantification of T cells that respond to a specific antigen but it also allows the detection of functionally relevant molecules upon specific stimulation of effector T cells. Although the tetramer staining method provides valuable information regarding the frequency of T cells (particularly CD8+ T cells), it needs to be combined with intracellular cytokine staining for the functional evaluation of T cells. However, the tetramer staining approach requires knowledge of the relevant epitope(s) and its restricting MHC molecule, limiting the use of this approach to the clinical setting. Thus, the ELISPOT is an attractive alternative because it is not limited by HLA restriction. Additionally, the low number of cells required to accurately assess T-cell activity (roughly tenfold less cell material than flow cytometry-based assays) as well as the high sensitivity and specificity of the assay makes the ELISPOT an optimal method for clinical monitoring [3], especially in clinical settings when the number of patient cells is limited (e.g., immunosuppressed subjects or pediatric patients). However, ELISPOT does not allow phenotypic characterization of antigen-stimulated T cells. Thus, magnetic isolation or depletion of T-cell subsets from peripheral blood mononuclear cells (PBMCs) is required to characterize antigen-specific CD8+ or CD4+ T-cell responses or both. Studies have shown that the ELISPOT assay provides reproducible results among different laboratories when the assay procedure and data analysis are standardized [46].

The interferon-gamma (IFN-γ) ELISPOT is the most widespread format used to measure and monitor antigen-specific T-cell responses induced by both prophylactic and therapeutic vaccine candidates. IFN-γ, a cytokine with antiviral, immunoregulatory, and antitumor properties [7], is produced by CD4+ T helper cell type 1 lymphocytes and CD8+ cytotoxic T lymphocytes (CTL) as part of the adaptive immune response. Additional cytokines, such as interleukin (IL)-2, IL-4, IL-5, IL-10, IL-12, IL-17, and tumor necrosis factor-α, can be evaluated by the ELISPOT assay, and kits are commercially available. Additionally, key molecules involved in the mechanism of cell-mediated cytotoxicity, such as granzyme B and perforin, have also been evaluated in an ELISPOT platform providing a more comprehensive evaluation of antigen-specific effector CTL functions [8].

A dual ELISPOT assay for the simultaneous detection of two cytokines, such as IFN-γ and IL-2, has been established, using a typical enzymatic approach [9] or using a specific fluorophore (FluoroSpot) [10]. An automated analysis of triple-color FluoroSpot for cytokine secretion has also been described [11]. A particular limitation is the availability of automated readers designed for the analysis of spots in three colors.

The goal of an efficient vaccine is to generate long-lived memory T cells capable of recognizing and rapidly expanding in response to infections [12]. Briefly, the three phases involved in the generation of a memory T-cell response are: activation and expansion, contraction, and differentiation into memory. After the initial phase of activation and expansion, the majority of effector T cells die, but the remaining 5–10% persist in the host and further mature into a stable pool of memory T cells. Such primed memory cells are maintained for a prolonged period of time after immunization and studies in humans indicate that memory responses can be maintained for decades [13, 14].

Memory T-cell populations are heterogeneous and consist of two broad categories of T-cell subsets that vary in their homing characteristics as well as their effector and proliferative functions. Expression of the lymph node homing receptors CCR7 and CD62L is the most frequently used to define the memory T-cell subsets. The effector memory T cells are typically CCR7 CD62L CD45RA and the central memory T cells are characterized as CCR7+ CD62L+ CD45RA [15]. Effector memory T cells traffic through nonlymphoid tissues and secrete mainly effector molecules (IFN-γ) and cytolytic molecules (perforin) while exhibiting reduce proliferative capacity. Central memory T cells express lymph node homing receptors and lack immediate effector function but exhibit robust proliferative capacity and elaborate effector molecules upon secondary stimulation.

This paper describes the principle of the ELISPOT assay as well as the types of ELISPOT assays used to enumerate and characterize human memory T cells based on IFN-γ production and discusses their application in the evaluation of immune correlates after vaccination.

2. The Principle of the ELISPOT Assay

The IFN-γ ELISPOT assay is carried out in commercially available synthetic membrane-bottomed 96-well plates. Plates are first coated with an IFN-γ-specific antibody (capture antibody). Then, PBMCs are added in the presence or absence of antigens and incubated for 18–24 hours. This incubation step allows responding cells to recognize the corresponding antigen and secrete IFN-γ, which is captured by the antibody. Cells are removed by washing and a biotinylated detection antibody directed to an epitope on IFN-γ distinct from that recognized by the capture antibody is added. Then, streptavidin conjugated with an enzyme (usually alkaline phosphatase or horseradish peroxidase) is added. Finally, a precipitated substrate for the streptavidin-linked enzyme is added, and plates are incubated until spots emerge. Each colored spot represents a single cell producing IFN-γ, and spot numbers are counted with an image-based spot reader with the accompanying analysis software. The readout of the assay is the number of IFN-γ secreting cells per number of cells plated. Figure 1(a) illustrates the steps involved in the ELISPOT assay.

Different cytokines have different secretion kinetics, which needs to be taken into account when measuring other cytokines rather than IFN-γ [3]. Cytokines such as IL-4, IL-5, or IL-17 require a longer (40 or 48 hours) activation period [16, 17]. While IFN-γ is an abundant cytokine, other cytokines (such as IL-2, IL-5, and IL-13) are produced by specific T cells present at a lower frequency [18].

ELISPOT assays are typically performed with total PBMCs, which contain sufficient antigen-presenting cells (APCs) for T-cell stimulation. Furthermore, depletion of specific T-cell subsets allows the characterization of antigen-specific T-cell responses. Commonly, T-cell depletion is performed using anti-CD4+ or anti-CD8+ antibody-coated immunomagnetic beads before starting the stimulation period with the specific antigens and corresponding controls.

The assay can be performed either with fresh or frozen PBMCs. After thawing, it is recommended to rest the cells before stimulation. In fact, an increase in background when cells are thawed just before plating and stimulation has been observed, while the lowest background levels are achieved by resting the cells from 6 hours to overnight [19]. In our laboratory, PBMCs are rested overnight (16–18 hours) in culture medium under humidified 37°C, 5% CO2 conditions. A resting period (at least 1 hour under humidified 37°C, 5% CO2 conditions) before stimulation should also be considered when working with freshly isolated PBMCs [19].

The choice of the antigen is critical. When proteins are used as antigens, APCs preferentially process the antigen(s) via the exogenous pathway of antigen presentation leading primarily to presentation of peptides on MHC class II molecules and stimulation of CD4+ T cells. However, a preincubation step prior plating the cells in the ELISPOT assay is required for optimal antigen presentation via MHC class II [20]. On the other hand, stimulation of CD8+ T cells requires the antigen to be processed via the endogenous pathway of antigen presentation, leading to the presentation of peptides on MHC class I molecules [21]. Peptides can be used as antigens to stimulate CD8+ T-cell responses through the direct binding to the MHC molecules avoiding the need for the endogenous pathway of antigen presentation. However, if peptides are of the proper length, they can be used to stimulate both CD8+ and CD4+ T-cell responses. Most immunologists use an entire protein-spanning mixture of overlapping peptides, presented by a variety of HLA alleles, for in vitro stimulation of T lymphocytes, allowing the HLA-unrestricted evaluation of T-cell responses. Sets of peptides, 15 amino acids in length with an 11 amino acid overlap, have been shown to represent a good compromise for stimulating both CD8+ and CD4+ T-cell responses in a number of applications [22, 23]. They are useful tools for screening and monitoring T-cell responses overtime. However, if a comparison of antigen-specific CD4+ versus CD8+ T-cell responses is required, shorter peptides (9 to 10 amino acids) are preferable to detect CD8+ T-cell responses [22].

Studies have shown that in general, IFN-γ spot forming cells are detected on stimulation with ≥0.1 μg/mL of peptide per pool and, when tested individually, a peptide concentration of 2 μg/mL is sufficient for the detection of antigen-specific T-cell responses [24]. In other studies, the final concentration of each peptide in a pool varied from 10 μg/mL [25] to 200 μg/mL [26]. No consensus on the optimal number of peptides that can be used per pool, which varies from 25 [24] to 123 [27], has been reached yet. A recent study suggests that using higher concentration and increased number of peptides per pool, the proliferation of antigen-specific CD8+ T cells may be inhibited [28]. In this study, peptide concentrations of 10 μg/mL showed a marked inhibition of proliferation, as compared to concentrations of 1 μg/mL [28]. The same event was observed when using pools containing 20 or 25 peptides with respect to pools containing 10 peptides [28]. Of note, peptides are usually dissolved in dimethyl sulfoxide (DMSO), which is toxic to cells at concentrations >0.5–1.0% in culture medium [24, 28].

Key controls are needed to measure antigen-specific T-cell responses. Negative control routinely consist of cells cultured in the absence of any stimulus, to assess background cytokine production. Stimulation with the polyclonal mitogen phytohemagglutinin (PHA) is the most common positive control for ELISPOT assays. CEF (cytomegalovirus, Epstein-Barr virus, influenza virus) peptide pools have been proposed as positive control as well as for optimizing and standardizing the assay [29]. These pools consist of peptides corresponding to a defined HLA class I-restricted T-cell epitope from each of these three viruses that are recognized by CD8+ T cells. There are also commercially available CEF peptide pools based on defined HLA class II-restricted T-cell epitopes.

Some empirical approaches have been proposed for determining an ELISPOT response [4, 30]. According to Dubey et al. [30] the cut-off for a positive response is ≥55 spots/million cells and ≥4-fold over the mean background (negative control). Similar criteria has also been proposed by other laboratories [19], in addition to defining a cut-off for the positive control (PHA, with at least >500 spots/million cells) and the mean background in negative wells (<30 spots/million cells). It should be noted that the positive criteria apply to the ELISPOT procedures and reagents that were used to validate them.

3. Types of ELISPOT Assays

Two types of ELISPOT assay, standard and cultured, have been designed to detect two different T-cell subsets. As mentioned before in the standard ELISPOT assay (also known as ex vivo ELISPOT assay), cells are incubated with the antigen for 18–24 hours and the cytokines that are released during that time by antigen-specific cells are captured by a monoclonal antibody allowing enumeration. This assay allows the measurement of T cells capable of immediate secretion of IFN-γ upon antigen stimulation. These cells are thought to represent mainly effector memory T cells.

Central memory T cells require antigenic restimulation to develop effector function, and the cultured ELISPOT assay is thought to comprise mainly these memory T cells, that is, central memory T cells [31]. The cultured ELISPOT assay requires a period of in vitro lymphocyte culture before the standard ELISPOT assay is performed (Figure 1(b)). Currently, we are performing this assay by culturing lymphocytes (5 × 105 cells/mL per well in a 48-well tissue culture plate) with specific antigens for 10 days allowing T cells to expand in response to the antigen. On days 3 and 7, half of the supernatant from each well is removed and replaced with fresh culture medium supplemented with 20 IU/mL recombinant human IL-2. After 10 days, cells from each well are harvested and washed before their use in the ELISPOT assay. Thus, antigen-stimulated cells are added to the ELISPOT plate and restimulated with the same antigen used for stimulation during the 10-day period. Variations in the cultured ELISPOT methodology (summarized in Table 1) include the length of the cultures, the tissue culture plate used, the concentration of IL-2 and the frequency with which it is replenished, and whether or not cultured cells are washed and rested before the performance of the ELISPOT assay. After subtracting from the number of spots in antigen-stimulated wells the number of spots in medium-stimulated wells, the results may be referred to as antigen-specific spot-forming cells per million input PBMCs [32], while others normalize the antigen-specific spots per million PBMCs to the proliferation index (number of antigen-stimulated cells divided by the number of medium-stimulated cells), to take into account the expansion of T cells during the culture [33, 34].

ReferenceLength of cultureSize of culture plateCells per well in culture plateConcentration and addition of IL-2Washing and resting cells before ELISPOT

Godkin et al. 2002 [37]12 days96-well plate 10 U/mL on days 3, 6, and 9Washing cells only
Pinder et al. 2004 [38]14 daysNot described 10 U/mL on days 5 and 10Washing cells only
Reece et al. 2004 [44]14 days48-well plate 10 U/mL on days 5 and 10Washing cells only
Keating et al. 2005 [32]10 days24-well plate 10 U/mL on days 3 and 7Washing and resting cells overnight
Goonetilleke et al. 2006 [35]11 to 13 daysNot described 1800 U/mL on days 3 and 7Washing and resting cells overnight
Calarota et al. 2008 [33]12 days24-well plate 10 U/mL on days 3 and 7Washing cells only
Todryk et al. 2009 [40]10 days24-well plate 100 U/mL on days 3 and 7Washing and resting cells overnight

It can be argued that the cultured ELISPOT assay increases the sensitivity of the standard ELISPOT assay by increasing the detection of low frequency antigen-specific T-cell responses [35, 36]. However, several studies have shown that the responses detected by ex vivo and cultured ELISPOT assays do not correlate with each other in response to HIV [33], EBV [34], hepatitis C virus [37], and malaria [38] antigens, by comparing the frequency of ex vivo response against the frequency of cultured response to the same antigen. These results suggest that different IFN-γ-producing cells are being evaluated, reflecting the different nature of these two assays.

It can also be argued that the stimulation protocol might induce in vitro priming of naïve T cells. However, we consider that it is unlikely to see significant de novo priming since the assay is of short duration (10 days) with no addition of peptide antigens other than the initial set-up, no addition of other exogenous cytokines apart from IL-2, and no enrichment of dendritic cells all of which are necessary for in vitro primary responses [39].

Evidence indicates that a different population of T cells, most likely central memory T cells that differentiate into effector T cells during the culture period, are measured by the cultured ELISPOT assay, as compared with the measurement of circulating effector memory T cells that are quantified by the standard ELISPOT. Todryk et al. [40] evaluated the effect of depletion of memory T-cell subsets on standard and cultured ELISPOT responses to recall antigens, such as influenza and purified protein derivative (PPD) of Mycobacterium tuberculosis. Results from these studies indicate that the depletion of CCR7+ or CD62L+ (central memory phenotype markers) cells reduced CD4+ and CD8+ T-cell responses detected by the standard ELISPOT, but the cultured ELISPOT responses were more dramatically reduced, indicating the predominant role of central memory T cells in the cultured ELISPOT response and also suggesting a role for this T-cell subset in the standard ELISPOT response. Godkin et al. [37] examined the effect of depletion of CCR7+ T cells on hepatitis C virus-specific standard and cultured ELISPOT responses. While depletion of CCR7+ T cells reduced the cultured ELISPOT response, the standard responses were only marginally affected by CCR7+ cell depletion, indicating that CCR7+ CD4+ T cells contribute substantially to the hepatitis C virus cultured memory cells but not to ex vivo responses.

Studies on an HIV-infected patient with residual HIV replication during antiretroviral treatment and with virus variants with several stop codons in the reverse transcriptase gene have shown robust Pol-specific cultured ELISPOT responses [41]. Furthermore, recent studies on elite controllers (HIV-infected individuals that control viral replication to levels below the limit of detection by standard clinical assays in the absence of antiretroviral treatment) indicate that expandable antigen-specific T cells measured by cultured ELISPOT from these individuals predominantly display a central memory phenotype [42]. Additionally, we have shown that standard and cultured ELISPOT responses to HIV [33] and EBV [34] antigens are different not only in frequency but also in the range of antigens recognized. Figure 2 dissects standard and cultured EBV-specific T-cell responses in an immunocompromised patient (an hematopoietic stem cell transplant recipient suffering from a EBV-associated posttransplant lymphoproliferative disorder) and a healthy subject with remote EBV infection. EBV-specific standard and cultured ELISPOT responses in the EBV seropositive healthy subject differed in both frequency and range of antigens recognized, and only few EBV-specific T-cell responses were detected in the patient with EBV-associated disease, which generally were of low frequency compared to the healthy subject.

4. Correlates of Immune Control

A better understanding of correlates of protective immunity against pathogens would be beneficial in designing vaccines. Studies performed in mice, infected with lymphocytic choriomeningitis virus or the intracellular bacterium Listeria monocytogenes, have shown that central memory T cells have a greater capacity than effector memory T cells to persist in vivo and are more efficient in mediating protective immunity because of their increased proliferative capacity [43]. Studies performed in humans have suggested that a CD4+ T-cell response to a conserved epitope in the circumsporozoite protein detected by cultured IFN-γ ELISPOT, rather than the ex vivo assay, correlated with protection from malaria infection and disease [44]. However, the protective capacity of different memory T-cell subsets may depend on the pathogen in question. Bachmann et al. [45] have reported that to protect mice against vaccinia virus, high numbers of effector memory T cells were required in peripheral tissue before viral challenge. Additionally, blood antigen-specific CD8+ effector memory T cells induced by immunizations with adenoviral and modified vaccinia Ankara vectors expressing pre-erythrocytic malaria antigens correlate with protection against malaria liver-stage infection [46].

Studies performed in rhesus macaques, immunized with plasmid DNA and replication defective adenoviral vectors encoding simian immunodeficiency virus (SIV) proteins and then challenged with pathogenic SIV, indicate that the preservation of vaccine induced antigen-specific central memory CD4+ T cells is essential for better outcome and survival following pathogenic SIV challenge [47]. Others suggest that central memory CD8+ T cells correlate with protection against SIV in rhesus macaques immunized with a vaccine candidate (DNA prime followed by a boost with the highly attenuated NYVAC-based SIV vaccine) [48]. It was found that the level of SIV replication following challenge exposure correlated inversely with the magnitude of vaccine-elicited SIV-specific central memory CD8+ T-cell responses but not with CD8+ effector memory T-cell responses [48]. However, it has been recently reported that SIV vaccines that include rhesus cytomegalovirus vectors elicited high-frequency SIV-specific effector memory T-cell responses at mucosal surfaces that control highly pathogenic SIV infection after mucosal challenge, suggesting a role for effector memory T cells as correlate of protection [49].

Studies have also shown that antigen-specific T-cell responses measured by cultured cellular assays, but not by standard ELISPOT, correlate with low viremia and high CD4+ counts in HIV-1-infected individuals naïve to antiretroviral therapy [33]. Yang et al. [50] investigated if hepatitis B-specific T-cell responses induced by DNA vaccination in 12 chronic hepatitis B carriers treated with lamivudine might be responsible for suppression of viral rebound after stopping the therapy. After discontinuation of the combined therapy, 6 patients showed undetectable viral load (virological responders) and the other 6 patients had high levels of viral load (nonvirological responders). Virological responders had higher antigen-specific ex vivo T-cell responses compared to nonvirological responders at the end or just before the discontinuation of the treatment, but only virological responders had detectable cultured ELISPOT responses for at least 40 weeks after the last vaccination. These data suggest that the cultured ELISPOT might be a better predictor of virological response than ex vivo ELISPOT [50]. T-cell responses to RD1 (region of difference 1 protein) antigens have been analyzed in patients with either severe or mild active tuberculosis as well as in successfully treated individuals (control subjects) and in subjects with negative tuberculin skin test results (negative control subjects) [51]. These studies have shown that in patients with severe active tuberculosis, both CD4+ T cell-mediated effector memory and central memory responses to the selected RD1 peptides were almost absent, while these responses were found in the majority of the patients with mild active tuberculosis. In contrast, recognition of the selected RD1 peptides was detected in the control subjects only by expanding the central memory T-cell pool [51].

Notably, the antigen-specific cultured ELISPOT response induced by a vaccine against malaria (heterologous DNA prime/boost with viral vectors) correlated significantly with the degree of protection against malaria sporozoite challenge. In contrast, antigen-specific standard ELISPOT responses did not predict protection against experimental malaria from sporozoite challenge [32]. This study established the cultured ELISPOT as a correlate of protection in malaria vaccine clinical trials [31].

The major goal in the field of T cell-inducing vaccine development (against, e.g., HIV, malaria, and tuberculosis) is the induction of long-term memory responses. In recent studies, cultured ELISPOT assays have proven to be a valuable tool for studying T-cell memory in HIV-1 vaccine trials [52, 53].

5. Conclusions

The ELISPOT is a straightforward, sensitive, specific, and widely utilized method for measuring T-cell responses after natural infection or vaccination. However, the frequency of T-cell responses obtained by the standard ELISPOT, quantifying effector memory T cells, does not correlate well with disease control or protection against challenge with some vaccine candidates. The cultured ELISPOT, on the other hand, quantifying central memory T cells, correlates with slow disease progression in natural infection and immune protection with several experimental vaccines. Thus, the two types of ELISPOT assays provide different information regarding T-cell-mediated immunity.


This work was supported by the Ministero della Salute, Fondazione IRCCS Policlinico San Matteo Ricerca Corrente Grant no. 80207.


  1. C. C. Czerkinsky, L. A. Nilsson, and H. Nygren, “A solid-phase enzyme-linked immunospot (ELISPOT) assay for enumeration of specific antibody-secreting cells,” Journal of Immunological Methods, vol. 65, no. 1-2, pp. 109–121, 1983. View at: Google Scholar
  2. C. Czerkinsky, G. Andersson, H.-P. Ekre, L.-A. Nilsson, L. Klareskog, and O. Ouchterlony, “Reverse ELISPOT assay for clonal analysis of cytokine production. I. Enumeration of gamma-interferon-secretion cells,” Journal of Immunological Methods, vol. 110, no. 1, pp. 29–36, 1988. View at: Publisher Site | Google Scholar
  3. P. V. Lehmann and W. Zhang, “Unique strengths of ELISPOT for T cell diagnostics,” Methods in Molecular Biology, vol. 792, pp. 3–23, 2012. View at: Publisher Site | Google Scholar
  4. J. H. Cox, G. Ferrari, S. A. Kalams et al., “Results of an ELISPOT proficiency panel conducted in 11 laboratories participating in international human immunodeficiency virus type 1 vaccine trials,” AIDS Research and Human Retroviruses, vol. 21, no. 1, pp. 68–81, 2005. View at: Publisher Site | Google Scholar
  5. W. Zhang, R. Caspell, A. Y. Karulin et al., “ELISPOT assays provide reproducible results among different laboratories for T-cell immune monitoring-even in hands of ELISPOT-inexperienced investigators,” Journal of Immunotoxicology, vol. 6, no. 4, pp. 227–234, 2009. View at: Publisher Site | Google Scholar
  6. M. J. Boaz, P. Hayes, T. Tarragona et al., “Concordant proficiency in measurement of T-cell immunity in human immunodeficiency virus vaccine clinical trials by peripheral blood mononuclear cell and enzyme-linked immunospot assays in laboratories from three continents,” Clinical and Vaccine Immunology, vol. 16, no. 2, pp. 147–155, 2009. View at: Publisher Site | Google Scholar
  7. K. Schroder, P. J. Hertzog, T. Ravasi, and D. A. Hume, “Interferon-γ: an overview of signals, mechanisms and functions,” Journal of Leukocyte Biology, vol. 75, no. 2, pp. 163–189, 2004. View at: Publisher Site | Google Scholar
  8. A. Malyguine, S. Strobl, L. Zaritskaya, M. Baseler, and K. Shafer-Weaver, “New approaches for monitoring CTL activity in clinical trials,” Advances in Experimental Medicine and Biology, vol. 601, pp. 273–284, 2007. View at: Publisher Site | Google Scholar
  9. S. Boulet, M. L. Ndongala, Y. Peretz et al., “A dual color ELISPOT method for the simultaneous detection of IL-2 and IFN-γ HIV-specific immune responses,” Journal of Immunological Methods, vol. 320, no. 1-2, pp. 18–29, 2007. View at: Publisher Site | Google Scholar
  10. N. Ahlborg and B. Axelsson, “Dual-and triple-color fluorospot,” Methods in Molecular Biology, vol. 792, pp. 77–85, 2012. View at: Publisher Site | Google Scholar
  11. J. A. Rebhahn, C. Bishop, A. A. Divekar et al., “Automated analysis of two- and three-color fluorescent Elispot (Fluorospot) assays for cytokine secretion,” Computer Methods and Programs in Biomedicine, vol. 92, no. 1, pp. 54–65, 2008. View at: Publisher Site | Google Scholar
  12. S. M. Kaech, E. J. Wherry, and R. Ahmed, “Effector and memory T-cell differentiation: implications for vaccine development,” Nature Reviews Immunology, vol. 2, no. 4, pp. 251–262, 2002. View at: Google Scholar
  13. E. Hammarlund, M. W. Lewis, S. G. Hansen et al., “Duration of antiviral immunity after smallpox vaccination,” Nature Medicine, vol. 9, no. 9, pp. 1131–1137, 2003. View at: Publisher Site | Google Scholar
  14. R. R. Amara, P. Nigam, S. Sharma, J. Liu, and V. Bostik, “Long-lived poxvirus immunity, robust CD4 help, and better persistence of CD4 than CD8 T cells,” Journal of Virology, vol. 78, no. 8, pp. 3811–3816, 2004. View at: Publisher Site | Google Scholar
  15. F. Sallusto, J. Geginat, and A. Lanzavecchia, “Central memory and effector memory T cell subsets: function, generation, and maintenance,” Annual Review of Immunology, vol. 22, pp. 745–763, 2004. View at: Publisher Site | Google Scholar
  16. C. R. Kreher, M. T. Dittrich, R. Guerkov, B. O. Boehm, and M. Tary-Lehmann, “CD4+ and CD8+ cells in cryopreserved human PBMC maintain full functionality in cytokine ELISPOT assays,” Journal of Immunological Methods, vol. 278, no. 1-2, pp. 79–93, 2003. View at: Publisher Site | Google Scholar
  17. J. T. Minang, I. Areström, and N. Ahlborg, “ELISpot displays a better detection over ELISA of T helper (Th) 2-type cytokine-production by ex vivo-stimulated antigen-specific T cells from human peripheral blood,” Immunological Investigations, vol. 37, no. 4, pp. 279–291, 2008. View at: Publisher Site | Google Scholar
  18. A. Letsch and C. Scheibenbogen, “Quantification and characterization of specific T-cells by antigen-specific cytokine production using ELISPOT assay or intracellular cytokine staining,” Methods, vol. 31, no. 2, pp. 143–149, 2003. View at: Publisher Site | Google Scholar
  19. H. Streeck, N. Frahm, and B. D. Walker, “The role of IFN-γ Elispot assay in HIV vaccine research,” Nature Protocols, vol. 4, no. 4, pp. 461–469, 2009. View at: Publisher Site | Google Scholar
  20. A. Schmittel, U. Keilholz, S. Bauer et al., “Application of the IFN-γ ELISPOT assay to quantify T cell responses against proteins,” Journal of Immunological Methods, vol. 247, no. 1-2, pp. 17–24, 2001. View at: Publisher Site | Google Scholar
  21. J. J. Monaco, “Pathways for the processing and presentation of antigens to T cells,” Journal of Leukocyte Biology, vol. 57, no. 4, pp. 543–547, 1995. View at: Google Scholar
  22. F. Kiecker, M. Streitz, B. Ay et al., “Analysis of antigen-specific T-cell responses with synthetic peptides—what kind of peptide for which purpose?” Human Immunology, vol. 65, no. 5, pp. 523–536, 2004. View at: Publisher Site | Google Scholar
  23. R. Draenert, M. Altfeld, C. Brander et al., “Comparison of overlapping peptide sets for detection of antiviral CD8 and CD4 T cell responses,” Journal of Immunological Methods, vol. 275, no. 1-2, pp. 19–29, 2003. View at: Publisher Site | Google Scholar
  24. N. D. Russell, M. G. Hudgens, R. Ha, C. Havenar-Daughton, and M. J. McElrath, “Moving to human immunodeficiency virus type 1 vaccine efficacy trials: defining T cell responses as potential correlates of immunity,” Journal of Infectious Diseases, vol. 187, no. 2, pp. 226–242, 2003. View at: Publisher Site | Google Scholar
  25. G. M. Lauer, M. Lucas, J. Timm et al., “Full-breadth analysis of CD8+ T-cell responses in acute hepatitis C virus infection and early therapy,” Journal of Virology, vol. 79, no. 20, pp. 12979–12988, 2005. View at: Publisher Site | Google Scholar
  26. M. M. Addo, X. G. Yu, A. Rathod et al., “Comprehensive epitope analysis of human immunodeficiency virus type 1 (HIV-1)-specific T-cell responses directed against the entire expressed HIV-1 genome demonstrate broadly directed responses, but no correlation to viral load,” Journal of Virology, vol. 77, no. 3, pp. 2081–2092, 2003. View at: Publisher Site | Google Scholar
  27. N. Jones, M. Eggena, C. Baker et al., “Presence of distinct subsets of cytolytic CD8+ T cells in chronic HIV infection,” AIDS Research and Human Retroviruses, vol. 22, no. 10, pp. 1007–1013, 2006. View at: Publisher Site | Google Scholar
  28. P. V. Suneetha, V. Schlaphoff, C. Wang et al., “Effect of peptide pools on effector functions of antigen-specific CD8+ T cells,” Journal of Immunological Methods, vol. 342, no. 1-2, pp. 33–48, 2009. View at: Publisher Site | Google Scholar
  29. J. R. Currier, E. G. Kuta, E. Turk et al., “A panel of MHC class I restricted viral peptides for use as a quality control for vaccine trial ELISPOT assays,” Journal of Immunological Methods, vol. 260, no. 1-2, pp. 157–172, 2002. View at: Publisher Site | Google Scholar
  30. S. Dubey, J. Clair, T.-M. Fu et al., “Detection of HIV vaccine-induced cell-mediated immunity in HIV-seronegative clinical trial participants using an optimized and validated enzyme-linked immunospot assay,” Journal of Acquired Immune Deficiency Syndromes, vol. 45, no. 1, pp. 20–27, 2007. View at: Publisher Site | Google Scholar
  31. A. Reyes-Sandoval, F. E. Pearson, S. Todryk, and K. Ewer, “Potency assays for novel T-cell-inducing vaccines against malaria,” Current Opinion in Molecular Therapeutics, vol. 11, no. 1, pp. 72–80, 2009. View at: Google Scholar
  32. S. M. Keating, P. Bejon, T. Berthoud et al., “Durable human memory T cells quantifiable by cultured enzyme-linked immunospot assays are induced by heterologous prime boost immunization and correlate with protection against malaria,” Journal of Immunology, vol. 175, no. 9, pp. 5675–5680, 2005. View at: Google Scholar
  33. S. A. Calarota, A. Foli, R. Maserati et al., “HIV-1-specific T cell precursors with high proliferative capacity correlate with low viremia and high CD4 counts in untreated individuals,” Journal of Immunology, vol. 180, no. 9, pp. 5907–5915, 2008. View at: Google Scholar
  34. S. A. Calarota, A. Chiesa, P. Zelini, G. Comolli, L. Minoli, and F. Baldanti, “Detection of Epstein-Barr virus-specific memory CD4+ T cells using a peptide-based cultured enzyme-linked immunospot assay,” Immunology, vol. 139, no. 4, pp. 533–544, 2013. View at: Google Scholar
  35. N. Goonetilleke, S. Moore, L. Dally et al., “Induction of multifunctional human immunodeficiency virus type 1 (HIV-1)-specific T cells capable of proliferation in healthy subjects by using a prime-boost regimen of DNA- and modified vaccinia virus Ankara-vectored vaccines expressing HIV-1 gag coupled to CD8+ T-cell epitopes,” Journal of Virology, vol. 80, no. 10, pp. 4717–4728, 2006. View at: Publisher Site | Google Scholar
  36. S. Campion, M. S. Cohen, A. J. McMichael, S. Galvin, and N. Goonetilleke, “Improved detection of latent Mycobacterium tuberculosis infection in HIV-1 seropositive individuals using cultured cellular assays,” European Journal of Immunology, vol. 41, no. 1, pp. 255–257, 2011. View at: Publisher Site | Google Scholar
  37. A. J. Godkin, H. C. Thomas, and P. J. Openshaw, “Evolution of epitope-specific memory CD4+ T cells after clearance of hepatitis C virus,” Journal of Immunology, vol. 169, no. 4, pp. 2210–2214, 2002. View at: Google Scholar
  38. M. Pinder, W. H. H. Reece, M. Plebanski et al., “Cellular immunity induced by the recombinant Plasmodium falciparum malaria vaccine, RTS,S/AS02, in semi-immune adults in The Gambia,” Clinical and Experimental Immunology, vol. 135, no. 2, pp. 286–293, 2004. View at: Publisher Site | Google Scholar
  39. J. M. Moser, E. R. Sassano, D. C. Leistritz et al., “Optimization of a dendritic cell-based assay for the in vitro priming of naïve human CD4+ T cells,” Journal of Immunological Methods, vol. 353, no. 1-2, pp. 8–19, 2010. View at: Publisher Site | Google Scholar
  40. S. M. Todryk, A. A. Pathan, S. Keating et al., “The relationship between human effector and memory T cells measured by ex vivo and cultured ELISPOT following recent and distal priming,” Immunology, vol. 128, no. 1, pp. 83–91, 2009. View at: Publisher Site | Google Scholar
  41. S. Paolucci, A. Foli, R. Gulminetti et al., “HIV-1 plasma variants encoding truncated reverse trancriptase (RT) in a patient with high RT-specific CD8+ memory T-cell response,” Current HIV Research, vol. 7, no. 3, pp. 302–310, 2009. View at: Publisher Site | Google Scholar
  42. Z. M. Ndhlovu, J. Proudfoot, K. Cesa et al., “Elite controllers with low to absent effector CD8+ T cell responses maintain highly functional, broadly directed central memory responses,” Journal of Virology, vol. 86, no. 12, pp. 6959–6969, 2012. View at: Google Scholar
  43. E. J. Wherry, V. Teichgräber, T. C. Becker et al., “Lineage relationship and protective immunity of memory CD8T cell subsets,” Nature Immunology, vol. 4, no. 3, pp. 225–234, 2003. View at: Publisher Site | Google Scholar
  44. W. H. H. Reece, M. Pinder, P. K. Gothard et al., “A CD4+ T-cell immune response to a conserved epitope in the circumsporozoite protein correlates with protection from natural Plasmodium falciparum infection and disease,” Nature Medicine, vol. 10, no. 4, pp. 406–410, 2004. View at: Publisher Site | Google Scholar
  45. M. F. Bachmann, P. Wolint, K. Schwarz, and A. Oxenius, “Recall proliferation potential of memory CD8+ T cells and antiviral protection,” Journal of Immunology, vol. 175, no. 7, pp. 4677–4685, 2005. View at: Google Scholar
  46. A. Reyes-Sandoval, D. H. Wyllie, K. Bauza et al., “CD8+ T effector memory cells protect against liver-stage malaria,” Journal of Immunology, vol. 187, no. 3, pp. 1347–1357, 2011. View at: Publisher Site | Google Scholar
  47. N. L. Letvin, J. R. Mascola, Y. Sun et al., “Preserved CD4+ central memory T cells and survival in vaccinated SIV-challenged monkeys,” Science, vol. 312, no. 5779, pp. 1530–1533, 2006. View at: Publisher Site | Google Scholar
  48. M. Vaccari, C. J. Trindade, D. Venzon, M. Zanetti, and G. Franchini, “Vaccine-induced CD8+ central memory T cells in protection from simian AIDS,” Journal of Immunology, vol. 175, no. 6, pp. 3502–3507, 2005. View at: Google Scholar
  49. S. G. Hansen, J. C. Ford, M. S. Lewis et al., “Profound early control of highly pathogenic SIV by an effector memory T-cell vaccine,” Nature, vol. 473, no. 7348, pp. 523–527, 2011. View at: Publisher Site | Google Scholar
  50. S.-H. Yang, C.-G. Lee, S.-H. Park et al., “Correlation of antiviral T-cell responses with suppression of viral rebound in chronic hepatitis B carriers: a proof-of-concept study,” Gene Therapy, vol. 13, no. 14, pp. 1110–1117, 2006. View at: Publisher Site | Google Scholar
  51. D. Goletti, O. Butera, F. Bizzoni, R. Casetti, E. Giradi, and F. Poccia, “Region of difference 1 antigen-specific CD4+ memory T cells correlate with a favorable outcome of tuberculosis,” Journal of Infectious Diseases, vol. 194, no. 7, pp. 984–992, 2006. View at: Publisher Site | Google Scholar
  52. N. Winstone, A. Guimarães-Walker, J. Roberts et al., “Increased detection of proliferating, polyfunctional, HIV-1-specific T cells in DNA-modified vaccinia virus Ankara-vaccinated human volunteers by cultured IFN-γ ELISPOT assay,” European Journal of Immunology, vol. 39, no. 4, pp. 975–985, 2009. View at: Publisher Site | Google Scholar
  53. J. Lisziewicz, N. Bakare, S. A. Calarota et al., “Single DermaVir immunization: dose-dependent expansion of precursor/memory T cells against all HIV antigens in HIV-1 infected individuals,” PLoS ONE, vol. 7, no. 5, Article ID e35416, 2012. View at: Google Scholar

Copyright © 2013 Sandra A. Calarota and Fausto Baldanti. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

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