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. 2016 Dec 22;6:39796. doi: 10.1038/srep39796

A20 Curtails Primary but Augments Secondary CD8+ T Cell Responses in Intracellular Bacterial Infection

Sissy Just 1, Gopala Nishanth 1,2, Jörn H Buchbinder 3, Xu Wang 1, Michael Naumann 4, Inna Lavrik 3, Dirk Schlüter 1,2,a
PMCID: PMC5177869  PMID: 28004776

Abstract

The ubiquitin-modifying enzyme A20, an important negative feedback regulator of NF-κB, impairs the expansion of tumor-specific CD8+ T cells but augments the proliferation of autoimmune CD4+ T cells. To study the T cell-specific function of A20 in bacterial infection, we infected T cell-specific A20 knockout (CD4-Cre A20fl/fl) and control mice with Listeria monocytogenes. A20-deficient pathogen-specific CD8+ T cells expanded stronger resulting in improved pathogen control at day 7 p.i. Imaging flow cytometry revealed that A20-deficient Listeria-specific CD8+ T cells underwent increased apoptosis and necroptosis resulting in reduced numbers of memory CD8+ T cells. In contrast, the primary CD4+ T cell response was A20-independent. Upon secondary infection, the increase and function of pathogen-specific CD8+ T cells, as well as pathogen control were significantly impaired in CD4-Cre A20fl/fl mice. In vitro, apoptosis and necroptosis of Listeria-specific A20-deficient CD8+ T cells were strongly induced as demonstrated by increased caspase-3/7 activity, RIPK1/RIPK3 complex formation and more morphologically apoptotic and necroptotic CD8+ T cells. In vitro, A20 limited CD95L and TNF-induced caspase3/7 activation. In conclusion, T cell-specific A20 limited the expansion but reduced apoptosis and necroptosis of Listeria-specific CD8+ T cells, resulting in an impaired pathogen control in primary but improved clearance in secondary infection.

CD8+ T cells are key players for the elimination of intracellular bacterial and viral pathogens. Upon stimulation with antigen, naïve pathogen-specific CD8+ T cells undergo rapid clonal expansion and effector CD8+ T cells (Teff) move to the site of infection, where they produce protective effector molecules and kill infected cells1. Following the peak of the primary CD8+ T cell response, typically around day 7, a contraction phase is induced, leading to massive cell death of Teff 2. Only 5–10% of the original pool of pathogen-specific CD8+ T cells survive and form a pool of long-living memory CD8+ T cells (Tmem)3. Upon rechallenge with the same pathogen, CD8+ Tmem cells rapidly expand and provide improved protection. The processes of (i) naïve CD8+ T cell activation and expansion, (ii) effector CD8+ T cell death during the contraction phase, and (iii) development and survival of memory CD8+ T cells are controlled by the NF-κB pathway, which is activated upon stimulation of the T cell receptor (TCR) by cognate antigen4,5,6,7. In addition, CD4+ T cells help during the acute phase of listeriosis by supporting the development of memory CD8+ T cells8,9.

A tight regulation of NF-κB activation is crucial for controlling the magnitude of the CD8+ T cell response and the development of different pathogen-specific CD8+ T cell subsets10. In intracellular bacterial infection, reduced activation of NF-κB results in impaired expansion of primary pathogen-specific CD8+ T cells11. However, prolonged stimulation of NF-κB also diminishes primary CD8+ T cell expansion by promoting their caspase-8 expression and apoptosis5. Interestingly, increased apoptosis of CD8+ T cells is mediated by CD95/CD95L interaction, which also regulates the development and maintenance of effector memory (TEM) versus central memory (TCM) CD8+ T cells5,12.

The ubiquitin modifying enzyme A20 plays a pivotal role as a negative feedback regulator of the canonical NF-κB signaling pathway upon activation of various cytokine and pattern recognition receptors13,14,15. A20 limits NF-κB activation by removing K63-linked polyubiquitin chains from signaling molecules including receptor-interacting serine/threonine-protein kinase 1 (RIPK1), RIPK2, TNF receptor-associated factor 6 (TRAF6) and IKK-γ (NEMO)16,17,18,19. In addition, A20 builds K48-polyubiquitin chains on RIPK1 inducing proteasomal degradation and indirectly inhibits signaling pathways by the suppression of NF-κB-induced gene expression16,20. A20 has also been reported to control the cell death program, in particular, of RIPK1/RIPK3-dependent necroptosis, by blocking ubiquitination of the RIPK1/3 complex21.

A20-deficient mice die prematurely of cachexia and tissue inflammation due to a hyperactivation of NF-κB22. In addition, selective deletion of A20 in dendritic cells23,24,25, myeloid cells26, B cells27,28,29, and astrocytes20 respectively, results in or exacerbates autoimmunity. In humans, polymorphisms of the A20-encoding Tnfaip3 gene predisposes to numerous diseases including autoimmune disorders30. In contrast, T cell-specific deletion of A20 protects from CD4+ T cell-mediated autoimmunity, which may be partially explained by increased cell death of activated A20-deficient CD4+ T cells due to caspase-independent and RIPK3-dependent necroptosis21. On the contrary, Giordano et al. have shown that deletion of A20 in T cells induced a more efficient anti-tumor CD8+ T cell response without evidence for an increased cell death of activated A20-deficient T cells31.

Here we investigated the role of A20 in the regulation of the CD8+ T cell response during intracellular bacterial infection. Upon infection with Listeria monocytogenes (Lm), T cell-specific A20 limited the magnitude of the primary effector CD8+ T cell response resulting in an impaired pathogen control. Notably, A20 reduced apoptosis and necroptosis of Lm-specific CD8+ T cells during primary T cell response, promoted survival of Tmem and improved protection against secondary infection.

Results

T cell numbers and activation in naïve mice

CD4-Cre A20fl/fl mice were born in normal Mendelian ratio and survived without any clinical signs of disease for at least one year (data not shown). In good agreement with Onizawa et al.21, splenic CD4+ and CD8+ T cells of CD4-Cre A20fl/fl mice were normal in numbers but slightly more activated, as indicated by increased CD69 expression, in comparison to A20fl/fl mice (Supplementary Fig. S1a–c). The small reduction of CD4+ T cell numbers may be caused by a reduction of invariant NK T cells, since A20 is required for the development of this subset of CD4+ T cells32.

Improved control of acute systemic listeriosis in CD4-Cre A20fl/fl mice

Since CD8+ T cells play a pivotal role in the clearance of Lm, we studied the effect of T cell-specific A20 on (i) pathogen control and (ii) the expansion and effector function of pathogen-specific CD8+ T cells in primary and secondary listeriosis according to the experimental outline illustrated in Fig. 1a.

Figure 1. Improved control of Listeria monocytogenes during primary infection but impaired clearance upon rechallenge in CD4-Cre A20fl/fl mice.

Figure 1

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(a) Experimental design: CD4-Cre A20fl/fl and A20fl/fl control mice were infected with Lm and spleens were analyzed at the indicated time points. Reinfection was performed 50 days after the primary infection. (b) CFU in spleen was determined at day 3, 7 and 14 after infection with Lm WT. (c) CFU in spleen after Lm OVA infection was determined at day 7 and 14 p.i. (d) CFU in spleen of Lm WT infected mice at day 50 and 3 days after reinfection at day 53. (e) CFU in spleen of Lm OVA infected mice at day 50 and 3 days after reinfection at day 53. Data are compiled of 3 independent experiments with 3-5 animals per group and experiment. Error bars indicate + SEM. Non-parametric Mann Whitney test, with *p < 0.05, **p < 0.01.

Upon primary infection with wildtype (Lm WT) and ovalbumin-expressing Lm (Lm OVA), pathogen control was significantly improved in CD4-Cre A20fl/fl mice in spleen (Fig. 1b,c) and liver (data not shown) at day 7 p.i. Up to day 50 p.i., Lm WT and Lm OVA were eliminated from spleens of both mouse strains. In sharp contrast to primary infection, reinfection on day 50 p.i. resulted in an impaired control of Lm WT and Lm OVA in CD4-Cre A20fl/fl mice (Fig. 1d,e).

In accordance with the kinetics of pathogen control, the relative and absolute numbers of Lm OVA-specific CD8+ T cells were significantly increased in CD4-Cre A20fl/fl mice at day 7 after infection with Lm OVA, i.e. the peak of the primary CD8+ T cell response (Fig. 2a,b). In contrast, the numbers of Lm OVA-specific IFN-γ-producing CD4+ T cells were identical in both mouse strains (Supplementary Fig. S3a) In parallel to pathogen clearance, Lm OVA-specific CD8+ T cells declined in both mouse strains gradually up to day 50 p.i. (Fig. 2a,b). However, this decline was stronger in CD4-Cre A20fl/fl mice and, upon secondary infection, the increase of Lm OVA-specific CD8+ T cells was significantly impaired as compared to A20fl/fl control mice. Upon reinfection of A20fl/fl control mice, the absolute number of pathogen-specific CD8+ T cells was increased as compared to the primary response. The number of pathogen-specific CD8+ T cells in CD4-Cre A20fl/fl mice, however, was reduced compared to the peak of the primary response (Fig. 2b).

Figure 2. Improved primary but impaired secondary CD8+ T cell response in CD4-Cre A20fl/fl mice.

Figure 2

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CD4-Cre A20fl/fl and A20fl/fl control mice were infected with a non-lethal dose of Lm OVA and CD8+ T cell response in spleen was analyzed at the indicated time points. (a) Representative dot plots and (b) absolute number of H2-Kb SIINFEKL pentamer+ CD8+ T cells after primary infection (day 0, 7 and 21 p.i.) and after reinfection (day 50 and 53 p.i.) with Lm OVA. (c) Representative dot plots and (d) absolute number of IFN-γ producing CD8+ T cells p.i. with Lm OVA and ex vivo restimulation with SIINFEKL peptide for 4 h in the presence of Brefeldin A. (e) IFN-γ-producing CD8+ T cells were gated and representative histograms of IFN-γ is displayed for the indicated time points after Lm OVA infection. (f) IFN-γ MFI from IFN-γ-producing CD8+ T cells. (g) Representative histograms and (h) granzyme B MFI of CD8+ T cells after Lm OVA infection and ex vivo restimulation with SIINFEKL peptide. (i) Representative histograms and (j) MFI of PD-1 expression on bulk CD8+ T cells (0 d.p.i.) or Lm OVA-specific CD8+ T cells (7, 21, 50 and 53 d.p.i.). A representative of 3 independent experiments is shown with 3 mice per group. Error bars indicate + SEM. Student’s t-test, *p < 0.05.

Consistently, relative and absolute numbers of IFN-γ-producing A20-deficient Lm OVA-specific CD8+ T cells were increased at day 7 p.i. (Fig. 2c,d). The numbers of protective IFN-γ-producing Lm OVA-specific CD8+ T cells declined over time in both mouse strains but IFN-γ-positive Lm OVA-specific CD8+ T cells were significantly reduced in CD4-Cre A20fl/fl at day 50 p.i. Importantly, the mean fluorescence intensity (MFI) of IFN-γ-producing Lm OVA-specific CD8+ T cells was significantly increased in CD4-Cre A20fl/fl mice at day 7 p.i. but rapidly declined thereafter resulting in a reduced IFN-γ production as compared to control mice at days 21 and 50 p.i. (Fig. 2e,f). Upon secondary infection, the relative and absolute numbers of IFN-γ-producing Lm OVA-specific CD8+ T cells strongly increased in A20fl/fl mice, whereas absolute numbers only slightly expanded in CD4-Cre A20fl/fl mice (Fig. 2c,d). Importantly, the IFN-γ MFI enhanced strongly in reinfected A20fl/fl mice but weakly increased in CD4-Cre A20fl/fl mice (Fig. 2e,f).

The kinetics of granzyme B-producing CD8+ T cells complemented the characteristic of the IFN-γ kinetics with increased numbers and MFI of granzyme B+ cells in CD4-Cre A20fl/fl mice in primary infection at day 7 p.i. but reduced numbers and MFI in reinfected mice at day 53 p.i. (Fig. 2g,h, Supplementary Fig. S2).

The reduced IFN-γ and granzyme B MFI of A20-deficient CD8+ T cells indicated a functional impairment in addition to reduced expansion. Therefore, we determined the expression of PD-1, which is upregulated on activated CD8+ T cells and can limit the function of pathogen-specific CD8+ T cells33. As illustrated in Fig. 2i,j, PD-1 was expressed on bulk CD8+ T cells in uninfected mice and also equally expressed on Lm OVA-specific CD8+ T cells of both strains at day 7 p.i. Thereafter, A20-competent Lm OVA-specific CD8+ T cells strongly downregulated PD-1 expression, whereas it further increased in A20-deficient CD8+ T cells. Upon reinfection, PD-1 MFI of A20-sufficient Lm OVA-specific CD8+ T cells strongly increased but declined in A20-deficient CD8+ T cells (Fig. 2i,j).

Next, we analyzed the Lm OVA-specific CD4+ T cell response, since CD4+ T cell help during acute infection by regulating CD8+ T cell responses in listeriosis8,9. In contrast to CD8+ T cells, numbers of Lm OVA-specific IFN- γ-producing CD4+ T cells were equally increased in both mouse strains (Supplementary Fig. S3a). Obar et al. reported that the expansion of Lm-specific CD8+ T cells in primary listeriosis may also depend on CD4+ T cell mediated upregulation of CD25 on CD8+ T cells early after infection (day 5 to 7 p.i.)34. Therefore, we determined the expression of CD25 on CD8+ T cells in acute listeriosis. As illustrated in Supplementary Fig. 3c, CD8+ T cells of both mouse strains equally up-regulated CD25 expression up to day 7 p.i.

In conclusion, Lm-specific CD4+ T cell responses were not significantly regulated by A20 indicating that the A20-dependent reduction of the primary but augmentation of the secondary Lm-specific CD8+ T cell response were CD4+ T cell independent.

A20 inhibits CD8+ T cell activation in vitro

In vitro stimulation of purified CD8+ T cells with anti-CD3/CD28 resulted in enhanced expression of A20 in control A20fl/fl cells (Supplementary Fig. S4a). The inhibitory role of A20 for T cell activation was further confirmed by an increased IκBα phosphorylation of A20-deficient CD8+ T cells as well as a slightly increased phosphorylation of p38 and ERK (Supplementary Fig. S4a). In accordance with our in vivo data, activation of A20-deficient T cells was augmented as illustrated by increased IFN-γ and TNF production (Supplementary Fig. S4b) and enhanced proliferation (Supplementary Fig. S4c,d).

Rapid decline of A20-deficient pathogen-specific effector, effector memory and central memory CD8+ T cells

Since CD4-Cre A20fl/fl mice developed an improved early primary CD8+ T cell response but failed to elicit the secondary response, we defined the time point of the loss of pathogen-specific A20-deficient CD8+ T cells by performing a detailed kinetic of Lm OVA-specific CD8+ T cells. After the peak of the primary Lm OVA-specific CD8+ T cell response at day 7 p.i., the relative (Fig. 3a) and absolute (Fig. 3b) numbers of pathogen-specific CD8+ T cells decreased in both strains of mice but the decline was significantly stronger in CD4-Cre A20fl/fl mice as compared to A20fl/fl control mice. Already at day 9 p.i., numbers of pathogen-specific CD8+ T cells were lower in CD4-Cre A20fl/fl mice. Thereafter, Lm OVA-specific CD8+ T cells declined with similar kinetic in both strains up to day 21 p.i., and absolute numbers of Lm OVA-specific CD8+ T cells remained consistently higher in A20fl/fl mice.

Figure 3. Reduced numbers of memory and memory-precursor CD8+ T cells in CD4-Cre A20fl/fl mice.

Figure 3

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CD4-Cre A20fl/fl and A20fl/fl control mice were infected with a non-lethal dose of Lm OVA and spleens were analyzed for Tmem formation at the indicated time points. (a) Kinetic of Lm OVA-specific CD8+ T cells, stained with H2-Kb SIINFEKL pentamer and gated on singlets and CD3+ CD8+ cells. (b) Absolute numbers of total (living, apoptotic and necroptotic) Lm OVA-specific CD8+ T cells. (c) Relative numbers of living (annexin−/7-AAD−) Lm OVA-specific CD8+ T cells. (d) Absolute numbers of living (annexin−/7-AAD−) Lm OVA-specific CD8+ T cells. (e) Representative dot plots with frequencies of Lm OVA-specific CD8+ SLEC (KLRG-1+ CD127−) and MPEC (KLRG-1− CD127+) were determined. (f) Absolute numbers of Lm OVA-specific CD8+ SLEC. (g) Absolute numbers of Lm OVA-specific CD8+ MPEC. (h) Representative dot plots with frequencies of Teff (CD62Llow and CD127low), TEM (CD62Llow and CD127high) and TCM (CD62Lhigh and CD127high) were determined at day 50 and 53 p.i. (i) Absolute numbers of Lm OVA-specific CD8+ Teff, TEM and TCM cells. Data are compiled of 2 independent experiments with 3–5 animals per group and experiment. Error bars indicate + SEM. Student’s t-test, *p < 0.05; **p < 0.01.

Further, we determined the relative (Fig. 3c) and absolute (Fig. 3d) number of living Lm OVA-specific CD8+ T cells by 7-AAD/annexin V staining during primary infection. The relative number of living Lm OVA-specific CD8+ T cells was significantly reduced in CD4-Cre A20fl/fl mice from day 7 to day 21 p.i. However, in CD4-Cre A20fl/fl mice, the absolute number of living cells (7-AAD− annexin V−) was significantly higher as compared to CD4-Cre A20fl/fl mice at day 7 p.i. but, thereafter, declined stronger in CD4-Cre A20fl/fl mice. At day 21 p.i., CD4-Cre A20fl/fl mice harbored only a very small number of living Lm OVA-specific CD8+ T cells (Fig. 3d).

Antigen-experienced CD8+ T cells are a heterogeneous group consisting of KLRG-1+ CD127− short-lived effector cells (SLEC) and KLRG-1− CD127+ memory precursor effector cells (MPEC)35,36. Therefore, we further investigated the development and kinetics of these cells. The relative and absolute numbers of Lm OVA-specific SLEC and MPEC were similar in both mouse strains at day 7 p.i. (Fig. 3e–g). Thereafter, SLEC declined in both strains but the relative number of SLEC remained higher in CD4-Cre A20fl/fl as compared to A20fl/fl mice (20.3 vs. 0.61% at day 21 p.i.). In contrast to SLEC, relative numbers of MPEC increased in both mouse strains but the increase was substantially higher in A20fl/fl mice (Fig. 3e). This resulted in a stable absolute number of MPEC in A20fl/fl mice, whereas they declined over time in CD4-CreA20fl/fl mice (Fig. 3g). Thus, at day 21 p.i., the Lm OVA-specific CD8+ T cell population of A20-sufficient animals contained mostly MPEC, while the A20-deficient Lm OVA-specific CD8+ T cell compartment consisted of a mixed population of SLEC and MPEC.

Next, we studied the relative and absolute numbers of Teff (CD62L− CD127−), TEM (CD62L− CD127+) and TCM (CD62L+ CD127+) at day 50 after primary infection and three days after reinfection (d53). At day 50 p.i., relative numbers of TEM were lower in CD4-Cre A20fl/fl mice and absolute numbers of all three subpopulations were significantly reduced in CD4-Cre A20fl/fl as compared to A20fl/fl mice (Fig. 3h,i). Upon reinfection, Teff increased strongly in A20fl/fl mice with an additional lower proliferation of TEM and TCM, whereas the increase of all CD8+ subpopulations was marginal in CD4-Cre A20fl/fl mice (Fig. 3i).

Taken together, A20 strongly supported the survival of Lm OVA-specific CD8+ T cells and the development of MPEC, TEM and TCM CD8+ T cells resulting in a stronger expansion of Teff upon reinfection.

A20-deficiency enhances necroptosis and apoptosis of pathogen-specific CD8+ T cells

The elimination of pathogen-specific CD8+ T cells was enhanced in CD4-Cre A20fl/fl mice, therefore, we investigated how A20 influenced cell death pathways. Due to the most substantial loss of pathogen-specific CD8+ T cells on day 7 and 11 p.i., we focused on these time points for the cell death analysis p.i. (Fig. 3a,b). Two major cell death programs apoptosis and programmed necrosis, also termed necroptosis, control the fate of T cells37. There are major differences in the morphology of the apoptotic vs. necroptotic cells that allow to distinguish between these two types of cell death. In particular, the necroptotic cells are typically swollen, while apoptotic cells undergo shrinkage during the course of cell death38. The identification of Lm OVA-specific CD8+ T cells undergoing apoptosis or necroptosis was performed by imaging flow cytometry (IFC), allowing the simultaneous analysis of a single cell by flow cytometry and microscopy to differentiate apoptosis from necroptosis38. Figure 4a illustrates the gating strategy for Lm OVA-specific CD8+ T cells (CD3+ CD8+ OVA-pentamer+) and the analysis of living (7-AAD− annexin V−), early apoptotic (7-AAD− annexin V+) and late apoptotic/necroptotic cells (7-AAD+ annexin V+) cell. Nuclear and membrane morphology of these cells were used to differentiate between living (Fig. 4B), early apoptotic (Fig. 4c), late apoptotic (Fig. 4d) and necroptotic cells (Fig. 4e).

Figure 4. Enhanced necroptosis and apoptosis of A20-deficient CD8+ T cells.

Figure 4

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CD4-Cre A20fl/fl and A20fl/fl control mice were infected with a sub-lethal dose of Lm OVA. On day 7 and 11 p.i., Lm OVA-specific CD8+ T cells were analyzed with IFC for apoptotic and necroptotic morphology. (a) IFC gating strategy for Lm OVA-specific CD8+ T cells and determination of double negative, annexin V+ (early apoptotic), and annexin V/7-AAD double positive cells. Double positive cells were further distinguished into late apoptotic and necroptotic cells. (b–e) Examples of microscopical analysis of cell morphology with IFC. (b) Living cells: negative for annexin V and 7-AAD. (c) Early apoptotic cells: annexin V+/7-AAD− with beginning of nucleus condensation and membrane blebbing. (d) Late apoptotic cells: annexin V+/7-AAD+ with condensed nuclei and membrane blebbing. (e) Necroptotic cells: annexin V+/7-AAD+ with swollen cell and nuclei. (f–g) Frequency of living, apoptotic (early and late stage) and necroptotic Lm OVA-specific CD8+ T cells in spleen at day 7 p.i. (f) and day 11 p.i. (g). A representative of 2 independent experiments is shown, with 3–4 mice per group. Error bars indicate + SEM. Student’s t-test, *p < 0.05; **p < 0.01.

At day 7 p.i., the relative number of living 7-AAD− annexin V− pathogen-specific CD8+ T cells with normal cellular morphology was approximately 30% in control mice but only 10% in CD4-Cre A20fl/fl mice (Fig. 4f). In control mice, equal percentages of apoptotic (7-AAD+/− annexin V+ with condensed nuclei and normal cell membrane) and necroptotic (7-AAD+ annexin V+ with swollen cell size and nuclei) Lm OVA-specific CD8+ T cells were present at day 7 p.i. (Fig. 4f). In contrast, relative numbers of Lm OVA-specific apoptotic cells were significantly reduced whereas necroptotic pathogen-specific CD8+ T cells were significantly increased in CD4-Cre A20fl/fl mice (Fig. 4f).

At day 11 p.i., relative numbers of Lm OVA-specific apoptotic and necroptotic cells were significantly increased in CD4-Cre A20fl/fl mice, whereas an increase of living Lm OVA-specific CD8+ T cells was observed in A20fl/fl mice (Fig. 4g).

Thus, the pool of pathogen-specific CD8+ T cells as shown in Figs 2a and 3b consists of living, apoptotic and necroptotic cells, and both cell death mechanisms contribute to the decline of pathogen-specific CD8+ T cells at the peak of the primary T cell response, which is controlled by A20.

A20-deficiency enhances apoptosis and necroptosis of CD8+ T cells in vitro

Down modulation of the primary T cell response has been reported to occur via CD95L/CD95 system and involves the activation of caspase-8, which further activates executioner caspases, including caspase-3, leading to apoptosis of the cell39. In addition to CD95, stimulation with TNF contributes to activation of cell death pathways. Stimulation of death receptors can result in the activation of a caspase-independent cell death pathway by the interaction and activation of RIPK1 and RIPK3, inducing necroptosis. Previously, it has been reported that anti-CD3/CD28 stimulation of A20-deficient CD4+ T cells results in an increased caspase-independent RIPK1/RIPK3-dependent necroptosis21. Since we detected both apoptosis and necroptosis of pathogen-specific CD8+ T cells in vivo, we further analyzed the mechanisms of how A20 regulates the cell death pathways in naïve CD8+ T cells in vitro.

Upon stimulation with anti-CD3/CD28, A20-competent and -deficient CD8+ T cells showed an increase in active caspase-3/7. This enhancement was significantly augmented in A20-deficient CD8+ T cells 72 h post stimulation (Fig. 5a). Upon additional stimulation with TNF, differences in active caspase-3/7 became significantly different even within 24 h (Fig. 5b). Notably, A20-deficient proliferating CD8+ T cells were characterized by increased caspase-3/7 activity compared to A20-competent CD8+ T cells (Fig. 5c).

Figure 5. A20-deficient T cells are highly susceptible to apoptosis and necroptosis in vitro.

Figure 5

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CD8+ T cells from CD4-Cre A20fl/fl and A20fl/fl control mice were isolated and stimulated with anti-CD3/CD28 and/or TNF, respectively, for the indicated time points. (a,b) Active caspase-3/7 was determined by flow cytometry using DEVD substrate after stimulation with (a) anti-CD3/CD28 only, or (b) anti-CD3/CD28 with TNF. (c) Dot Plots showing proliferation and caspase-3/7 activity after 72 h of stimulation. (d) Western blot analysis of full length caspase-8, cleaved caspase-8, full-length caspase-3 and cleaved caspase-3 after TCR or TNF stimulation, respectively. (e) Lysates from unstimulated and 48 h anti-CD3/CD28-stimulated CD8+ T cells were immunoprecipitated with anti-RIPK1. Protein concentrations were equalized by staining lysates for GAPDH. Beads plus lysate without antibody (B+L) and beads plus anti-RIPK1 without lysates (B+A) were used as controls. (f) CD8+ T cells were left untreated or stimulated with anti-CD3/CD28 for 72 h and IFC was performed. A representative of 2 independent experiments is shown, with 3 mice per group. Error bars indicate + SEM. Student’s t-test, *p < 0.05; **p < 0.01.

To further confirm that A20-deficiency augmented apoptosis of CD8+ T cells upon in vitro stimulation, we analyzed procaspase-3 and −8 cleavage by western blotting in T cells activated by anti-CD3/CD28 or TNF, respectively. As illustrated in Fig. 5d, the amounts of cleaved effector caspase-3 as well as procaspase-8 cleavage products p43 and p18 were enhanced in A20-deficient CD8+ T cells upon anti-CD3/CD28 and TNF stimulation, respectively.

To study the necroptosis pathway, we analyzed RIPK1/RIPK3 interactions. Upon stimulation with anti-CD3/CD28, RIPK1 immunoprecipitates of A20-competent and –deficient CD8+ T cells showed presence of RIPK3 (Fig. 5e) illustrating the formation of the RIPK1/RIPK3 necroptotic complexes and that, in addition to apoptosis, necroptosis is induced in anti-CD3/CD28-activated CD8+ T cells.

To further analyze the regulation of cell death pathways by A20, we quantified the number of necroptotic and apoptotic CD8+ T cells by IFC analysis (Fig. 5f). In unstimulated cells the frequency of necroptotic, but not apoptotic, CD8+ T cells was increased in A20-deficient cells, corresponding to the RIPK1/RIPK3 complex formation and the absence of cleaved caspase-3 and −8 in A20-deficient CD8+ T cells (Fig. 5d,e). Upon anti-CD3/CD28 stimulation, necroptosis and apoptosis were strongly induced in A20-sufficient CD8+ T cells, but were even more prominent in A20-deficient CD8+ T cells, indicating that A20 regulates both cell death pathways.

A20 inhibits CD95 expression and CD95L-induced apoptosis of CD8+ T cells

CD95 can contribute to the induction of two opposing processes: the activation or cell death of pathogen-specific CD8+ T cells. Among other factors the outcome of CD95 ligation depends on (i) the status of the T cell, i.e. naïve, resting or activated T cell, (ii) the amount of CD95 and CD95 agonists and (iii) the strength of CD95 signaling37,39,40,41,42,43. Therefore, we analyzed whether Lm OVA-specific CD8+ T cells upregulated CD95 during listeriosis and whether this process was regulated by A20.

Already at day 7 p.i., A20-deficient Lm OVA-specific CD8+ T cells expressed more CD95 than A20-competent T cells. In both genotypes, CD95 expression increased over time but was significantly higher in A20-deficient pathogen-specific CD8+ T cells at all time points up to day 21 p.i. (Fig. 6a). In parallel to CD95 upregulation, caspase-3/7 activity was significantly upregulated in A20-deficient Lm OVA-specific CD8+ T cells at the peak of the primary CD8+ T cell response at day 7 p.i, increased drastically on day 11 p.i. and was maintained on high levels at all later time points. In contrast, only a slight increase of caspase-3/7 activity was observed in A20fl/fl control mice (Fig. 6b).

Figure 6. A20 reduces CD95 expression by inhibition of NF-κB activation.

Figure 6

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(a) Histograms display MFI of CD95 ex vivo on Lm OVA-specific CD8+ T cells at the indicated time points p.i. (b) Ex vivo kinetic of active caspase-3/7 in Lm OVA-specific CD8+ T cells at the indicated time points p.i. (c) CD8+ T cells were in vitro stimulated with anti-CD3/CD28 and flow cytometric analysis for CD95 was performed at the indicated time points. (d) Frequency of living cells was determined after in vitro stimulation with anti-CD3/CD28. Cell death was determined by flow cytometry, staining for annexin V and 7-AAD. (e) T cells were stimulated with anti-CD3/CD28, treated with IKK-inhibitor or were left untreated. mRNA was isolated and levels of CD95 were determined. (f) CD8+ T cells were stimulated in vitro with anti-CD3/CD28 and recombinant CD95L for the indicated time points. Active caspase 3/7 was measured using DEVD substrate. (g) Frequency of living cells was determined after CD8+ T cells were stimulated with CD95L for 2 h. To inhibit apoptosis, Z-VAD-FMK was added prior to the stimulation. (h) Active caspase-3/7 was determined before and after AICD. (a,b) Cells were gated on singlets and H2-Kb SIINFEKL+ CD8+ T cells. A representative of 2 independent experiments is shown, with 3 mice per group. Error bars indicate + SEM. (a–d,f,h) Student’s t-test. (e,g) Tukey’s multiple comparison test; *p < 0.05; **p < 0.01.

Furthermore, in vitro stimulation of naïve CD8+ T cells with anti-CD3/CD28 induced a significantly stronger upregulation of CD95 in A20-deficient as compared to A20-sufficient CD8+ T cells (Fig. 6c). In parallel, numbers of living annexinV−/7-AAD− CD8+ T cells declined in both groups but the reduction was significantly stronger in the absence of A20 (Fig. 6d).

Activation of NF-κB induces expression of CD95 and, thus, the increased cell death of A20-deficient CD8+ T cells may be partially mediated by augmented CD95 expression due to the lack of NF-κB inhibition44. To test this hypothesis, we analyzed the role of A20 for NF-κB-mediated induction of CD95 expression in CD8+ T cells. Upon stimulation with anti-CD3/CD28 A20-deficient CD8+ T cells CD95 mRNA increased 2.7 fold, whereas in A20-sufficient CD8+ T cells upregulation of CD95 mRNA was only 1.8 fold (Fig. 6e). Importantly, inhibition of NF-κB activation by an IKK-inhibitor prevented upregulation of CD95 mRNA in both A20-deficient and -sufficient cells and completely abolished differences between the two genotypes (Fig. 6e).

To test the functional importance of the increased NF-κB-dependent CD95 expression of A20-deficient CD8+ T cells, we treated anti-CD3/CD28-stimulated CD8+ T cells with CD95L. In fact, CD95L stimulation induced a significantly stronger activation of caspase-3/7 in A20-deficient CD8+ T cells within 24 h (Fig. 6f). Noteworthy, inhibition of the caspase activity by Z-VAD-FMK significantly reduced cell death of A20-deficient and competent CD95L-stimulated CD8+ T cells (Fig. 6g) illustrating that CD95-induced apoptosis of activated CD8+ T cells is strongly reduced by A20. However, even in Z-VAD-FMK-treated cells, the frequency of living cells was still significantly reduced in A20-deficient cells, indicating that in addition to apoptosis, other cell death pathways, e.g. necroptosis, are augmented in CD95-stimulated A20-deficient CD8+ T cells.

In vivo, CD95-mediated activation induced cell death (AICD) plays a critical role in the contraction phase of pathogen-specific T cells to maintain immune homeostasis after clearance of the infection37. To study whether A20 regulates AICD, we stimulated CD8+ T cells with anti-CD3/CD28 and IL-2 for 2 days, expanded the cells in IL-2 containing medium for another 3 days before restimulation with anti-CD3. As illustrated in Fig. 6h, anti-CD3 restimulation induced a much stronger caspase-3/7 activity in A20-deficient CD8+ T cells compared to A20-competent cells demonstrating that A20 suppresses AICD.

Taken together, these data delineate a crucial inhibitory role of A20 on CD95-induced CD8+ T cell apoptosis.

Discussion

The control of intracellular infections requires complex dynamics of protective pathogen-specific CD8+ T cells including (i) the expansion of effector CD8+ T cells upon primary infection, (ii) the contraction of these effector T cells after pathogen clearance, (iii) the development and persistence of memory CD8+ T cells, and (iv) the rapid expansion of memory CD8+ upon reinfection. Here, we show that A20 regulates all of these different CD8+ T cell responses and plays an opposing role for pathogen-specific CD8+ T cell responses in the course of an intracellular bacterial infection. At the peak of the primary CD8+ T cell response (day 7 p.i.), the A20-deficient effector CD8+ T cell response was greatly augmented with increased numbers of IFN-γ-producing and cytotoxic granzyme B+ CD8+ T cells resulting in an improved clearance of the pathogen. Thereafter, A20-deficient pathogen-specific CD8+ T cells failed to establish a protective memory T cell pool, resulting in a diminished control of Listeria upon secondary infection.

Recently, Drennan et al. demonstrated that splenic CD8+ T cells of naïve mice express A20 in vivo32. In accordance with Giordano et al.31, we also observed a low baseline expression of A20 in unstimulated CD8+ T cells in vitro, which was upregulated in TCR-stimulated CD8+ T cells, and restricted activation of NF-κB and MAP kinases, CD8+ T cell proliferation, and IFN-γ and TNF production. Of note, numbers of IFN-γ-producing as well as granzyme B+ pathogen-specific CD8+ T cells were significantly increased in CD4-Cre A20fl/fl mice at the peak of the primary T cell response. In naïve CD4-Cre A20fl/fl mice, the absence of this suppressive activity of A20 may account for the increased activation of CD4+ and CD8+ T cells as evidenced by elevated CD69 expression. Of note, the increased activation of T cells, which has also been detected by Giordano et al.31, did not result in a spontaneous inflammatory disease of CD4-Cre A20fl/fl mice (our unpublished data), which has also not been described before31,32. This may be explained by the fact that cytokine production of CD4+ (IFN-γ, IL-2) and CD8+ T cells (IFN-γ, granzyme B) was not increased in naïve CD4-Cre as compared to A20fl/fl mice. This is in contrast to mouse strains with deletion of A20 in B cells, dendritic cells and macrophages, respectively, which all develop severe spontaneous inflammatory diseases23,24,25,26,45 and indirectly argues for a specific deletion of A20 in T cells of CD4-Cre A20fl/fl mice.

Although activation of NF-κB is required for the development of an efficient primary effector CD8+ T cell response as well as for the development of memory T cells4,7,46, the excessive and prolonged activation of this signaling pathway can either lead to the development of autoimmunity or the induction of programmed cell death47. We considered two major hypotheses, how the increased NF-κB activation of A20-deficient pathogen-specific CD8+ T cells might cause reduced numbers of TEM and TCM: (i) A20 regulates the development of SLEC and MPEC CD8+ T cells, and (ii) A20 inhibits cell death and enables persistence of CD8+ T cells. A detailed analysis of the in vivo kinetics of Lm-specific T cells revealed that absolute numbers of Lm-specific CD8+ TCM and TEM, respectively, were increased in CD4-Cre A20fl/fl mice at the peak of the primary CD8+ T cell response. However already at day 9 p.i., absolute numbers of Lm OVA-specific CD8+ T cells were reduced in CD4-Cre A20fl/fl mice due to an increased cell death of A20-deficient T cells. In particular, the maintenance of MPEC was severely impaired in A20-deficient CD8+ T cells, which might contribute to the impaired pathogen-specific CD8+ TEM and TCM response of CD4-Cre A20fl/fl mice. Noteworthy, Lm OVA-specific CD8+ T cells increased 15-fold upon reinfection (Fig. 3h,i), whereas A20-deficient Lm OVA-specific CD8+ T cells increased only 3-fold within three days after reinfection. Although this marginal increase may indicate an impaired expansion of A20-deficient Lm-specific CD8+ T cells, this assumption has to be regarded with caution, since the significantly lower number of pathogen-specific A20-deficient memory CD8+ T cells at day 50 p.i. will result per se and A20-independent in lower numbers of pathogen-specific CD8+ T cell three days after reinfection. In addition to the development and expansion of CD8+ T cell subsets, A20 regulated the functional activity of Lm OVA-specific CD8+ T cells. At the peak of the primary CD8+ T cell response, IFN-γ and granzyme B production of A20-deficient CD8+ T cells was augmented, whereas it was diminished thereafter and also upon reinfection. This corresponds to the increased absolute number of living A20-deficient Lm OVA-specific CD8+ T cells at day 7 p.i. and the reduced number of A20-deficient pathogen-specific CD8+ T cells from day 9 p.i onward (Fig. 3d). At day 7 p.i., the co-inhibitory receptor PD-1 was equally induced in both A20-deficient competent and –deficient Lm OVA-specific CD8+ T cells, which is consistent with the induction of this inhibitory receptor during CD8+ T cell activation48. However, in contrast to A20-competent CD8+ T cells, A20-deficient Lm OVA-specific CD8+ T cells failed to downregulate and even further upregulated PD-1 after the elimination of Listeria. We speculate that this elevated PD-1 expression of A20-deficient CD8+ T cells contributed to their functional impairment, since PD-1 causes the characteristic exhausted phenotype, i.e. poor cell division and cytokine production of CD8+ T cells in chronic viral infections49. At present we do not know whether A20 reduces PD-1 expression by a direct or indirect mechanism but so far it has not been reported that A20 regulates the transcriptional repressor Blimp-1, which directly silences PD-1 expression in the late phases of acute effector CD8+ T cell responses50.

CD8+ T cell memory and SLEC development and, thereby, protective secondary CD8+ T cell responses are dependent on CD4+ T cell help in listeriosis8,9,34. Since the frequency of Lm-specific IFN-γ+ and IL-2+ CD4+ T cells were not affected by A20-deficiency in primary and secondary listeriosis, and, additionally, CD25 expression of CD8+ T cells was upregulated normally in CD8+ T cells, a diminished CD4+ T cell response is unlikely to cause the A20-dependent effects in CD8+ T cells. Although we do not formally show that the defective CD8+ T cell response of A20-deficient CD8+ T cells is only caused by the intrinsic A20-defect, these in vivo data in combination with the corresponding in vitro phenotype of A20-deficient CD8+ T cells strongly suggest that A20 expression in CD8+ T cells is the major factor causing the altered CD8+ T cell response in listeriosis.

Apoptosis and necroptosis are two different forms of programmed cell death, which can be induced in T cells by stimulation with TNF51 and activation of the death receptor CD9552. Whereas apoptosis is mediated by the activation of caspases including caspase-3 and −7, necroptosis depends on the formation and activation of a RIPK1/RIPK3 complex53. Several studies suggest that the contraction of pathogen-specific CD8+ T cells after primary infection is caused by apoptosis, which is in part dependent on CD95 stimulation54,55. However, quantitative in vivo data on the respective role of apoptosis and necroptosis for the contraction of pathogen-specific CD8+ T cells have not been reported so far, which is largely based on the difficulty to unequivocally differentiate and quantify apoptosis and necroptosis in vivo. Of note, apoptosis and necroptosis are morphologically distinct. Apoptotic cells are characterized by phosphatidylserine exposure on the cell surface followed by membrane blebbing, nuclear fragmentation, decreased cellular volume and formation of apoptotic bodies56. In contrast, necroptotic cells include early plasma membrane rupture followed by rapid cytoplasmic and nuclear swelling and organelle breakdown38. Based on these differences, we used IFC, which combines quantitative single cell microscopy with flow cytometry and quantified ex vivo apoptotic and necroptotic pathogen-specific CD8+ T cells. Of note, this analysis included all OVA257–264-specific CD8+ T cells including living, apoptotic and necroptotic cells.

In A20-competent pathogen-specific CD8+ T cells, necroptosis and apoptosis equally contributed to the cell death and contraction of the Lm OVA-specific CD8+ T cell pool. In A20-deficient pathogen-specific CD8+ T cells necroptosis was enhanced but apoptosis was decreased at the peak of the T cell response (day 7 p.i.), indicating a role of A20 as a suppressor of necroptosis. However, at day 11 p.i. more apoptosis and necroptosis of Lm-specific CD8+ T cells were observed in CD4-Cre A20fl/fl mice. Thus, A20 inhibits both cell death pathways in pathogen-specific CD8+ T cells in vivo, although the relative effect of A20 on each of these two pathways may be regulated by additional factors including CD95 expression (Fig. 6a).

The FlowSight analysis of Lm OVA-specific CD8+ T cells (Fig. 4) revealed that (i) the total number of H2-Kb SIINFEKL-specific CD8+ T cells as displayed in Figs 2a and 3b was composed of living, apoptotic and necroptotic cells and (ii) the relative numbers of necroptotic and/or apoptotic pathogen-specific CD8+ T cells were increased and relative numbers of living cells reduced in CD4- Cre A20fl/fl mice (Fig. 4f). The increased numbers of apoptotic/necroptotic A20-deficient pathogen-specific CD8+ T cells explain why the initially significantly elevated absolute numbers of A20-deficient Lm OVA-specific CD8+ T cells (day 7 p.i.) rapidly declined and were already significantly reduced at day 11 p.i. as compared to A20-competent CD8+ T cells. Only at day 7 p.i., the absolute numbers of living A20-deficient Lm OVA-specific CD8+ T cells were increased as compared to A20-competent CD8+ T cells, which coincides with the increased absolute numbers of IFN-γ and granzyme B producing pathogen-specific CD8+ T cells and the significantly reduced bacterial load in CD4-Cre A20fl/fl mice at this time point.

A recent in vitro study of Onizawa et al. also identified A20 as a suppressor of necroptosis in CD4+ T cells acting at ubiquitination of RIPK321. However, in contrast to our data on pathogen-specific CD8+ T cells, A20-deficiency of CD4+ T cells completely abolished apoptosis. In contrast, Drennan et al. demonstrated that A20-deficiency resulted in an increased cell death of invariant NK T cells due to apoptosis but not necroptosis32. At present, the discrepant results concerning the induction and A20-mediated regulation of apoptosis and necroptosis of CD8+ (our study), CD4+ T cells21 and invariant NK T cells32 are unresolved but may be explained by intrinsic cell-type specific differences between these two T cell subsets.

Under in vitro conditions, flow cytometry and IFC in combination with western blot analysis of active caspase-3 and −8 and RIPK1/RIPK3 complex formation further illustrated that irrespective of A20 expression, TCR-stimulated CD8+ T cells underwent both apoptosis and necroptosis. A20-deficient CD8+ T cells were more prone to necroptosis, which is mediated via RIPK1/RIPK3 complex formation. A20 removes Lys63 chains from RIPK1 via its OTU domain and promotes the addition of degradative polyubiquitin chains on RIPK1 via its zinc-finger 4 motif. Deubiquitination of RIPK1/RIPK3 complex is a key step towards necroptosis induction, therefore, the molecular mechanisms of the effects observed in our work require further intensive investigations. Furthermore, upon in vitro stimulation with anti-CD3/CD28, both necroptosis and apoptosis were increased in A20-deficient CD8+ T cells.

T cell apoptosis can be induced by several factors including TNF and CD95L. In accordance, stimulation with TNF induced active caspase-3 and −8 and stimulation with CD95L mediated active caspase-3/7 expression in naïve CD8+ T cells in vitro. Importantly, both pathways were augmented in A20-deficient cells indicating that in vivo cell death of Lm-specific CD8+ T cells is most probably mediated by several mechanisms including TNF and CD95.

It has been shown before that the contraction and survival of pathogen-specific CD8+ T cells is independent of CD95 expression57,58, while the maintenance of functional Lm-specific CD8+ T cells requires CD95/CD95L interactions in a CD8+ T cell extrinsic manner12. However, an increased expression of CD95, as observed in mice with constitutive NF-κB activation5, may contribute to an increased cell death of Lm-specific CD8+ T cells, which is in line with CD95 as an apoptosis inducing factor upon NF-κB-mediated activation44. Corresponding to the increased NF-κB activation (Supplementary Fig. S4A), A20-deficient CD8+ T cells strongly upregulated CD95 upon activation and inhibition of NF-κB completely abolished the increased CD95 expression of TCR-stimulated A20-deficient CD8+ T cells. Collectively, the published and our data are compatible with the assumption that depending on the strength of CD95 stimulation and signaling, cell death of activated T cells may be induced59. In listeriosis, A20-deficient Lm OVA-specific CD8+ T cells expressed more CD95 and active caspase-3/7 as compared to A20-sufficient CD8+ T cells. Thus, the increased cell death of A20-deficient pathogen-specific CD8+ T cells may partially depend on CD95 in combination with other cell death inducing mechanisms including the TNF receptor pathway.

In vivo, pathogen-specific CD8+ T cells may encounter repetitively cognate-antigen presenting cells. Therefore, a balance between TCR-induced expansion and CD95-mediated AICD of CD8+ T cells is mandatory. Experimentally, AICD can be mimicked in vitro by repetitive TCR stimulation and, here, we demonstrate a significantly increased caspases-3/7 activity in A20-deficient CD8+ T cells upon AICD-induction. Thus, AICD will further contribute to the impaired survival of A20-deficient Lm-specific CD8+ T cells.

Taken together, A20 limits the magnitude of the primary pathogen-specific CD8+ T cell response but strengthens memory T cell survival and secondary CD8+ T cell responses by restricting the apoptosis- and necroptosis-mediated contraction of the pathogen-specific CD8+ T cell pool.

Materials and Methods

Mice

A20fl/fl mice on a C57BL/6 background as described before were crossed with CD4-Cre mice to obtain CD4-Cre A20fl/fl mice25. Genotyping was done by PCR of tail DNA with primers for CD4-Cre and A20fl/fl.

Ethics statement

Animal experiments were performed according to the German Animal Welfare Act (Deutsches Tierschutzgesetz) and approved by local authorities (Landesverwaltungsamt Sachsen-Anhalt; file number: 42502-2-994). All efforts were made to minimize suffering and surgery was performed after euthanization.

Infection of mice and determination of colony forming units

Listeria monocytogenes wild type (Lm WT, EGD strain) and the ovalbumin expressing strain L. monocytogenes (Lm OVA) were used in the experiments, respectively. Listeria were grown in brain heart infusion broth and aliquots of log-pase cultures were stored at −80 °C. Fresh log-phase cultures were prepared from frozen stocks and mice were infected i.v. via the tail vein with 1 × 104 Lm WT and 5 × 104 Lm OVA, respectively, diluted in 200 μl sterile PBS (pH 7.4). Reinfection was performed with 1 × 106 CFU Lm WT or Lm OVA, respectively, at day 50 p.i. Bacterial dose used for infections was confirmed by plating an inoculum on brain heart infusion agar and counting colonies after incubation at 37 °C for 24 h.

To determine CFUs in infected mice, animals were sacrificed at the indicated time points p.i., spleens were homogenized with sterile tissue grinders. Tenfold serial dilutions of the homogenates were plated on brain heart infusion agar. Bacterial colonies were counted after incubation at 37 °C for 24 h and the number of bacteria per spleen was calculated.

Flow cytometry

Single cell suspensions from spleen, liver, lymph nodes and thymus were prepared as described before11. Cells were stained for 30 min at 4 °C using mouse specific fluorochrome-labled antibodies for CD3 (145-2C11), CD4 (RM4-5), CD8 (53-6.7), CD45 (30-F11) for T cells, F4/80 (BM8), CD11b (M1/70), Ly-6G (1A8) and Ly-6C (HK1.4) for macrophages, neutrophils and monocytes, CD11c (N418) for dendritic cells and NK1.1 (PK136) for NK cells from BioLegend or eBioscience after blocking with anti-CD16/32 (BioLegend). Ag-specific CD8+ T cells were detected using PE-conjugated H2-Kb SIINFEKL pentamer (ProImmune). CD8+ T cells were further characterized by staining with antibodies for CD69, CD62L (MEL-14), CD44 (IM7), CD127 (A7R34), KLRG-1 (2F1/KLRG1), PD-1 (RMP1-14) and CD95 (SA367H8). Intracellular staining was performed by ex vivo stimulation for 4 h at 37 °C with the ovalbumin-specific peptide H-SIINFEKL-OH (SIINFEKL) for CD8+ T cells or H-ISQAVHAAHAEINEAGR-OH (OVACD4) for CD4+ T cells in presence of Brefeldin A (BioLegend) and stained for IFN-γ (XMG1.2), granzyme B (NGZB) or IL-2 from BioLegend with the Intracellular Fixation & Permeabilization Kit from eBioscience. Cytokine concentration in supernatant and serum was determined using cytometric bead array (BD Bioscience). Active caspase-3/7 measurement was performed using CellEvent Caspase-3/7 Green ReadyProbes (Life Technologies). Flow cytometric analysis was performed on a BD FACS CANTO II (BD Bioscience) and analyzed with FlowJo X software (Milltenyi).

In vitro T cell stimulation

CD8+ T cells were isolated from spleen and lymph nodes from A20fl/fl and CD4-Cre A20fl/fl mice with Mouse CD8+ T cell Isolation Kit (Stemcell Technologies) according to manufacturer’s instruction. Cells were stimulated in RPMI 1640 medium supplemented with L-glutamine, 10% FCS, 100 U/ml penicillin, 100 μg/ml streptomycin, 1 mM sodium pyruvate, 1% non-essential amino acids, 50 μM β-mercaptoethanol (all from Life Technologies) and 5 mM HEPES (Biochrom) in the presence of 1 μg/ml plate-bound anti-CD3 and 2 μg/ml soluble anti-CD28 (both from BioLegend) for 3 days.

Proliferation was analyzed by staining cells with carboxyfluorescein succinimidyl ester (CFSE, BioLegend) before stimulation.

For active caspase-3/7 measurement, CD8+ T cells were stimulated for the indicated time points with the addition of 20 ng/ml TNF or recombinant CD95L (50 ng/ml).

Activation induced cell death (AICD)

CD8+ T cells were isolated and stimulated in the presence of 1 μg/ml plate-bound anti-CD3, 2 μg/ml soluble anti-CD28 and 20 ng/ml IL-2. On day 2, cells were harvested and expanded in IL-2-containing medium for 3 days. On day 5, T cells were restimulated for 6 h with 10 μg/ml plate-bound anti-CD3.

Imaging Flow Cytometry (IFC)

Spleen cells were isolated as described before and stained for H2-Kb SIINFEKL-specific CD8+ T cells. Cells were washed and resuspended in annexin staining buffer and stained with annexin V (Life Technologies) and 7-AAD (BioLegend).

For in vitro analysis cells were stimulated for three days with anti-CD3/CD28 or 2 h with CD95L, respectively. Staining was done as described above. IFC was performed on Amnis FlowSight Imaging Flow Cytometer (EMD Millipore).

Western Blot analysis

Cells were isolated from spleen and lymph nodes, sorted for total T cells (Stemcell Technologies) and resuspended in radioimmunoprecipitation assay (RIPA) buffer with protease inhibitor after stimulation with anti-CD3/CD28 or TNF for the indicated time points. After 30 min incubation on ice the lysates were centrifuged and the supernatant was collected. Protein concentration was measured with Bradford Assay and was calculated based on a standard dilution using photometer. For SDS-PAGE, sample buffer was added to lysates in a 1:5 dilution and incubated for 5 min at 95 °C. After gel run proteins were transferred on PVDF membranes and afterwards incubated in TBST with 5% BSA or Blotto B. Antibodies against A20 (A-12) from Santa Cruz, p-IκBα (Ser32), p-p38 (Thr180/Tyr182), p-ERK (Thr202/Tyr204), Caspase-3 and Caspase-8 (cell signaling) were used. Blots were developed using ECL Plus Kit (Thermo Scientific).

Immunoprecipitation

Proteins from unstimulated and anti-CD3/CD28-stimulated CD8+ T cells were isolated as described before and pre-incubated with Sepharose beads (GE Healthcare Bio-Sciences) for 30 min at 4 °C with agitation to block unspecific binding. Afterwards samples were centrifuged for 10 min at 10,000 × g. Equal amounts of protein were incubated with anti-RIPK1 antibody (cell signaling) over night at 4 °C on a rocker. Sepharose beads were added to the samples and incubated over night at 4 °C on a rocker. To collect the immunoprecipitate, the samples were centrifuged and the beads were washed 3 times with PBS to remove unspecific binding. After the last washing step, beads were resuspended in 1X lane marker reducing sample buffer and incubated at 99 °C for 3 min. The beads were removed by centrifugation and western blot analysis was performed as described above.

RT-qPCR

T cells were stimulated for the indicated time points and total RNA was isolated according to manufacturer’s instruction (RNeasy kit, Qiagen). cDNA synthesis was generated using SuperScript reverse transcriptase kit (Invitrogen) and qPCR was performed for HPRT and CD95 with TaqMan probes (Applied Biosystems) on a Lightcycler 480 system (Roche). Data were analyzed according to ΔΔ cycle threshold method.

Statistical analysis

All data are represented as mean + SEM and statistical analysis was performed as indicated in the figure legends, respectively, using GraphPad Prism 5 software. A p value of <0.05 was considered statistically significant.

Additional Information

How to cite this article: Just, S. et al. A20 Curtails Primary but Augments Secondary CD8+ T Cell Responses in Intracellular Bacterial Infection. Sci. Rep. 6, 39796; doi: 10.1038/srep39796 (2016).

Publisher's note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary Material

Supplementary Material
srep39796-s1.doc (448.5KB, doc)

Acknowledgments

The authors thank Nadja Schlüter and Annette Sohnekind for technical assistance. This study was supported by a grant from the Deutsche Forschungsgemeinschaft (SFB 854, TP5) to MN and DS (http://www.sfb854.de/).

Footnotes

Author Contributions S.J., G. N., J.B. and X.W. conducted the experiment. M.N., I.L. and D.S. designed the experiments. S.J., M.N., I.L. and D.S. wrote the paper.

References

  1. Zhang N. & Bevan M. J. CD8(+) T cells: foot soldiers of the immune system. Immunity 35, 161–8 (2011). [DOI] [PMC free article] [PubMed] [Google Scholar]
  2. Porter B. B. & Harty J. T. The onset of CD8+ -T-cell contraction is influenced by the peak of Listeria monocytogenes infection and antigen display. Infect. Immun. 74, 1528–1536 (2006). [DOI] [PMC free article] [PubMed] [Google Scholar]
  3. Kaech S. M., Hemby S., Kersh E. & Ahmed R. Molecular and functional profiling of memory CD8 T cell differentiation. Cell 111, 837–851 (2002). [DOI] [PubMed] [Google Scholar]
  4. Hettmann T., Opferman J. T., Leiden J. M. & Ashton-Rickardt P. G. A critical role for NF-κB transcription factors in the development of CD8+ memory-phenotype T cells. Immunol. Lett. 85, 297–300 (2003). [DOI] [PubMed] [Google Scholar]
  5. Krishna S. et al. Chronic activation of the kinase IKKβ impairs T cell function and survival. J. Immunol. 189, 1209–1219 (2012). [DOI] [PMC free article] [PubMed] [Google Scholar]
  6. Schulze-Luehrmann J. & Ghosh S. Antigen-Receptor Signaling to Nuclear Factor κB. Immunity 25, 701–715 (2006). [DOI] [PubMed] [Google Scholar]
  7. Zehn D., King C., Bevan M. J. & Palmer E. TCR signaling requirements for activating T cells and for generating memory. Cell. Mol. Life Sci. 69, 1565–1575 (2012). [DOI] [PMC free article] [PubMed] [Google Scholar]
  8. Shedlock D. J. & Shen H. Requirement for CD4 T Cell Help in Generating Functional CD8 T Cell Memory. Science (80-.) 300, 337–339 (2003). [DOI] [PubMed] [Google Scholar]
  9. Sun J. C. & Bevan M. J. Defective CD8 T Cell Memory Following Acute Infection Without CD4 T Cell Help. Science (80-.) 300, 339–343 (2003). [DOI] [PMC free article] [PubMed] [Google Scholar]
  10. Li Q., Verma I. M. & Pines & NF-κB Regulation in the Immune System. Nat. Rev. Immunol. 2, 725–734 (2002). [DOI] [PubMed] [Google Scholar]
  11. Sakowicz-Burkiewicz M. et al. Protein Kinase C-theta Critically Regulates the Proliferation and Survival of Pathogen-Specific T Cells in Murine Listeriosis. J. Immunol. 180, 5601–5612 (2008). [DOI] [PubMed] [Google Scholar]
  12. Dudani R., Russell M., van Faassen H., Krishnan L. & Sad S. Mutation in the Fas pathway impairs CD8+ T cell memory. J. Immunol. 180, 2933–41 (2008). [DOI] [PMC free article] [PubMed] [Google Scholar]
  13. Opipari a W., Boguski M. S. & Dixit V. M. The A20 cDNA induced by tumor necrosis factor alpha encodes a novel type of zinc finger protein. J. Biol. Chem. 265, 14705–14708 (1990). [PubMed] [Google Scholar]
  14. Liew F. Y., Xu D., Brint E. K. & O’Neill L. A. J. Negative regulation of Toll-like receptor-mediated immune responses. Nat. Rev. Immunol. 5, 446–458 (2005). [DOI] [PubMed] [Google Scholar]
  15. Shi C.-S. & Kehrl J. H. TRAF6 and A20 regulate lysine 63-linked ubiquitination of Beclin-1 to control TLR4-induced autophagy. Sci. Signal. 3, ra42 (2010). [DOI] [PMC free article] [PubMed] [Google Scholar]
  16. Wertz I. E. et al. De-ubiquitination and ubiquitin ligase domains of A20 downregulate NF-κB signalling. Nature 430, 694–699 (2004). [DOI] [PubMed] [Google Scholar]
  17. Hitotsumatsu O. et al. The ubiquitin-editing enzyme A20 restricts nucleotide-binding oligomerization domain containing 2-triggered signals. Immunity 28, 381–90 (2008). [DOI] [PMC free article] [PubMed] [Google Scholar]
  18. Heyninck K. & Beyaert R. The cytokine-inducible zinc finger protein A20 inhibits IL-1-induced NF-kappaB activation at the level of TRAF6. FEBS Lett. 442, 147–50 (1999). [DOI] [PubMed] [Google Scholar]
  19. Skaug B. et al. Direct, noncatalytic mechanism of IKK inhibition by A20. Mol. Cell 44, 559–71 (2011). [DOI] [PMC free article] [PubMed] [Google Scholar]
  20. Wang X. et al. Astrocytic A20 ameliorates experimental autoimmune encephalomyelitis by inhibiting NF-κB- and STAT1-dependent chemokine production in astrocytes. Acta Neuropathol. 3, 711–724 (2013). [DOI] [PubMed] [Google Scholar]
  21. Onizawa M. et al. The ubiquitin-modifying enzyme A20 restricts ubiquitination of the kinase RIPK3 and protects cells from necroptosis. Nat. Immunol. 16, 618–627 (2015). [DOI] [PMC free article] [PubMed] [Google Scholar]
  22. Lee E. G. et al. Failure to regulate TNF-induced NF-kappaB and cell death responses in A20-deficient mice. Science 289, 2350–2354 (2000). [DOI] [PMC free article] [PubMed] [Google Scholar]
  23. Hammer G. E. et al. Expression of A20 by dendritic cells preserves immune homeostasis and prevents colitis and spondyloarthritis. Nat. Immunol. 12, 1184–1193 (2011). [DOI] [PMC free article] [PubMed] [Google Scholar]
  24. Kool M. et al. The ubiquitin-editing protein A20 prevents dendritic cell activation, recognition of apoptotic cells, and systemic autoimmunity. Immunity 35, 82–96 (2011). [DOI] [PubMed] [Google Scholar]
  25. Xuan N. T. et al. A20 expression in dendritic cells protects mice from LPS-induced mortality. Eur. J. Immunol. 45, 818–828 (2014). [DOI] [PubMed] [Google Scholar]
  26. Matmati M. et al. A20 (TNFAIP3) deficiency in myeloid cells triggers erosive polyarthritis resembling rheumatoid arthritis. Nat. Genet. 43, 908–12 (2011). [DOI] [PubMed] [Google Scholar]
  27. Chu Y. et al. B cells lacking the tumor suppressorTNFAIP3/A20 display impaired differentiation and hyperactivation and cause inflammation and autoimmunity in aged mice. Blood 117, 2227–2236 (2011). [DOI] [PubMed] [Google Scholar]
  28. Hövelmeyer N. et al. A20 deficiency in B cells enhances B-cell proliferation and results in the development of autoantibodies. Eur. J. Immunol. 41, 595–601 (2011). [DOI] [PubMed] [Google Scholar]
  29. Tavares R. M. et al. The Ubiquitin Modifying Enzyme A20 Restricts B Cell Survival and Prevents Autoimmunity. Immunity 33, 181–191 (2010). [DOI] [PMC free article] [PubMed] [Google Scholar]
  30. Ma A. & Malynn B. A. A20: linking a complex regulator of ubiquitylation to immunity and human disease. Nat. Rev. Immunol. 12, 774–785 (2012). [DOI] [PMC free article] [PubMed] [Google Scholar]
  31. Giordano M. et al. The tumor necrosis factor alpha-induced protein 3 (TNFAIP3, A20) imposes a brake on antitumor activity of CD8 T cells. Proc. Natl. Acad. Sci. USA 3, 1–6 (2014). [DOI] [PMC free article] [PubMed] [Google Scholar]
  32. Drennan M. B. et al. NKT sublineage specification and survival requires the ubiquitin-modifying enzyme TNFAIP3/A20. J. Exp. Med. jem.20151065 doi: 10.1084/jem.20151065 (2016). [DOI] [PMC free article] [PubMed] [Google Scholar]
  33. Keir M. E., Butte M. J., Freeman G. J. & Sharpe A. H. PD-1 and its ligands in tolerance and immunity. Annu Rev Immunol 26, 677–704 (2008). [DOI] [PMC free article] [PubMed] [Google Scholar]
  34. Obar J. J. et al. CD4+ T cell regulation of CD25 expression controls development of short-lived effector CD8+ T cells in primary and secondary responses. Proc. Natl. Acad. Sci. USA 107, 193–8 (2010). [DOI] [PMC free article] [PubMed] [Google Scholar]
  35. Sarkar S. et al. Functional and genomic profi ling of eff ector CD8 T cell subsets with distinct memory fates. J.Exp.Med 205, 625–640 (2008). [DOI] [PMC free article] [PubMed] [Google Scholar]
  36. Joshi N. S. et al. Article Inflammation Directs Memory Precursor and Short-Lived Effector CD8+ T Cell Fates via the Graded Expression of T-bet Transcription Factor. Immunity 27, 281–295 (2007). [DOI] [PMC free article] [PubMed] [Google Scholar]
  37. Krammer P. H., Arnold R. & Lavrik I. N. Life and death in peripheral T cells. Nat. Rev. Immunol. 7, 532–542 (2007). [DOI] [PubMed] [Google Scholar]
  38. Pietkiewicz S., Schmidt J. H. & Lavrik I. N. Quantification of apoptosis and necroptosis at the single cell level by a combination of Imaging Flow Cytometry with classical Annexin V/propidium iodide staining. J. Immunol. Methods 423, 99–103 (2015). [DOI] [PubMed] [Google Scholar]
  39. Krueger A., Fas S. C., Baumann S. & Krammer P. H. The role of CD95 in the regulation of peripheral T-cell apoptosis. Immunol. Rev. 193, 58–69 (2003). [DOI] [PubMed] [Google Scholar]
  40. Paulsen M. et al. Modulation of CD4+ T-cell activation by CD95 co-stimulation. Cell Death Differ. 18, 619–631 (2011). [DOI] [PMC free article] [PubMed] [Google Scholar]
  41. Lavrik I. N. & Krammer P. H. Regulation of CD95/Fas signaling at the DISC. Cell Death Differ. 19, 36–41 (2012). [DOI] [PMC free article] [PubMed] [Google Scholar]
  42. Schleich K. et al. Stoichiometry of the CD95 Death-Inducing Signaling Complex: Experimental and Modeling Evidence for a Death Effector Domain Chain Model. Mol. Cell 47, 306–319 (2012). [DOI] [PubMed] [Google Scholar]
  43. Lavrik I. N. et al. Analysis of CD95 Threshold Signaling: Triggering of CD95 (Fas/APO-1) at low concentrations primarily results in survival signaling. J. Biol. Chem. 282, 13664–13671 (2007). [DOI] [PubMed] [Google Scholar]
  44. Chan H., Bartos D. P. & Owen-Schaub L. B. Activation-dependent transcriptional regulation of the human Fas promoter requires NF-κB p50-p65 recruitment. Mol Cell Biol 19, 2098–2108 (1999). [DOI] [PMC free article] [PubMed] [Google Scholar]
  45. Boone D. L. et al. The ubiquitin-modifying enzyme A20 is required for termination of Toll-like receptor responses. Nat. Immunol. 5, 1052–1060 (2004). [DOI] [PubMed] [Google Scholar]
  46. Gerondakis S. & Siebenlist U. Roles of the NF-κB pathway in lymphocyte development and function. Cold Spring Harb. Perspect. Biol. 2, 1–29 (2010). [DOI] [PMC free article] [PubMed] [Google Scholar]
  47. Chandok M. R. & Farber D. L. Signaling control of memory T cell generation and function. Semin. Immunol. 16, 285–293 (2004). [DOI] [PubMed] [Google Scholar]
  48. Agata Y. et al. Expression of the PD-1 antigen on the surface of stimulated mouse T and B lymphocytes. Int. Immunol. 8, 765–772 (1996). [DOI] [PubMed] [Google Scholar]
  49. Wherry E. J., Blattman J. N., Murali-krishna K., Most R. Van Der & Ahmed R. Viral Persistence Alters CD8 T-Cell Immunodominance and Tissue Distribution and Results in Distinct Stages of Functional Impairment. J. Virol. 77, 4911–4927 (2003). [DOI] [PMC free article] [PubMed] [Google Scholar]
  50. Lu P. et al. Blimp-1 represses CD8 T cell expression of PD-1 using a feed-forward transcriptional circuit during acute viral infection. J. Exp. Med. 211, 515–527 (2014). [DOI] [PMC free article] [PubMed] [Google Scholar]
  51. Lu J. V. et al. Complementary roles of Fas-associated death domain (FADD) and receptor interacting protein kinase-3 (RIPK3) in T-cell homeostasis and antiviral immunity. Proc. Natl. Acad. Sci. USA 108, 15312–7 (2011). [DOI] [PMC free article] [PubMed] [Google Scholar]
  52. Pasparakis M. & Vandenabeele P. Necroptosis and its role in inflammation. Nature 517, 311–320 (2015). [DOI] [PubMed] [Google Scholar]
  53. Silke J., Rickard J. A. & Gerlic M. The diverse role of RIP kinases in necroptosis and inflammation. Nat. Immunol. 16, 689–697 (2015). [DOI] [PubMed] [Google Scholar]
  54. Mogil R. J. et al. Fas (CD95) participates in peripheral T cell deletion and associated apoptosis in vivo. Int. Immunol. 7, 1451–8 (1995). [DOI] [PubMed] [Google Scholar]
  55. Renno T., Hahne M., Tschopp J. & MacDonald H. R. Peripheral T cells undergoing superantigen-induced apoptosis in vivo express B220 and upregulate Fas and Fas ligand. J. Exp. Med. 183, 431–437 (1996). [DOI] [PMC free article] [PubMed] [Google Scholar]
  56. Henry C. M., Hollville E. & Martin S. J. Measuring apoptosis by microscopy and flow cytometry. Methods 61, 90–7 (2013). [DOI] [PubMed] [Google Scholar]
  57. Zimmermann C., Rawiel M., Blaser C., Kaufmann M. & Pircher H. Homeostatic regulation of CD8+ T cells after antigen challenge in the absence of Fas (CD95). Eur. J. Immunol. 26, 2903–10 (1996). [DOI] [PubMed] [Google Scholar]
  58. Reich A., Körner H., Sedgwick J. D. & Pircher H. Short paper Immune down-regulation and peripheral deletion of CD8 T cells does not require TNF receptor-ligand interactions nor CD95 (Fas, APO-1). Eur. J. Immunol. 678–682 (2000). [DOI] [PubMed] [Google Scholar]
  59. Paulsen M. & Janssen O. Pro- and anti-apoptotic CD95 signaling in T cells. Cell Commun. Signal. 9, 7 (2011). [DOI] [PMC free article] [PubMed] [Google Scholar]

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