Myc controls the metabolic reprogramming that supports effector T cell differentiation. The expression of Myc is regulated by the T cell antigen receptor (TCR) and pro‐inflammatory cytokines such as interleukin‐2 (IL‐2). We now show that the TCR is a digital switch for Myc mRNA and protein expression that allows the strength of the antigen stimulus to determine the frequency of T cells that express Myc. IL‐2 signalling strength also directs Myc expression but in an analogue process that fine‐tunes Myc quantity in individual cells via post‐transcriptional control of Myc protein. Fine‐tuning Myc matters and is possible as Myc protein has a very short half‐life in T cells due to its constant phosphorylation by glycogen synthase kinase 3 (GSK3) and subsequent proteasomal degradation. We show that Myc only accumulates in T cells exhibiting high levels of amino acid uptake allowing T cells to match Myc expression to biosynthetic demands. The combination of digital and analogue processes allows tight control of Myc expression at the population and single cell level during immune responses.
See also: C Chou & T Egawa (August 2015)
A combination of digital and analogue processes allows tight control of Myc expression at the population and single cell level during T lymphocyte immune responses and matches Myc expression to biosynthetic demands.
The T cell antigen receptor operates an essential on/off switch for Myc expression. The strength of the antigen stimulus determines the frequency of immune‐activated T cells that express Myc.
Myc protein has a very short half‐life in activated T cells because it is constantly phosphorylated by glycogen synthase kinase 3 (GSK3) and targeted for proteasomal degradation.
The constant high level of Myc proteolysis means Myc protein levels can only be sustained in T cells that have high rates of amino acid uptake and protein synthesis.
The post‐transcriptional control of Myc protein is used by pro‐inflammatory cytokines such as interleukin‐2 to fine‐tune Myc levels in individual T cells.
The fine‐tuning of Myc levels in individual T cells is shown to be important for a key aspect of T cell metabolism: the regulated uptake of transferrin that ensures immune‐activated T cells have sufficient iron.
Immune‐activated T lymphocytes undergo rapid clonal expansion and differentiation into effector subpopulations. Activated T cells also strikingly increase nutrient uptake and lipid and protein biosynthesis. Naïve T lymphocytes thus have low rates of amino acid and glucose uptake and use oxidative phosphorylation to efficiently metabolise glucose to generate ATP. In contrast, effector T cells upregulate amino acid and glucose uptake and switch to metabolising glucose through glycolysis (Greiner et al, 1994; Fox et al, 2005; Jacobs et al, 2008); they also metabolise glutamine to pyruvate and lactate via glutaminolysis (Brand et al, 1984; Newsholme et al, 1985). These changes in T cell metabolism are necessary to support the production of the cytokines and cytolytic effector molecules that are essential for T cell immune responses (Pollizzi & Powell, 2014).
One key controller of metabolic reprogramming in T cells is Myc (myelocytomatosis oncogene, c‐Myc). In the absence of Myc, mature T cells cannot respond to antigen receptor engagement to increase the expression of glucose and glutamine transporters and fail to initiate glycolysis or glutamine catabolism (Wang et al, 2011a). Myc loss also has a global impact on the T cell transcriptome. Myc may thus have multiple transcriptional targets or act to amplify expression of active genes in T cells (Nie et al, 2012). The importance of Myc in T lymphocytes is also exemplified by its role in T cell development in the thymus (Dose et al, 2006, 2009; Mycko et al, 2009; Jiang et al, 2010) and by its key role in T cell malignancies. For example, elevated Myc expression is observed in most cases of T cell acute lymphoblastic leukaemia (T‐ALL), either as a consequence of a chromosomal translocation event (t(8;14)(q24;q11)) that places Myc under the control of the TCR alpha chain promoter (Erikson et al, 1986; Charrin, 1996) or more commonly as a consequence of Notch mutations that lead to transcriptional activation of Myc (Weng et al, 2004, 2006; Palomero et al, 2006).
It was recognised many years ago that upregulation of Myc mRNA accompanied T cell activation (Reed et al, 1987; Kelly & Siebenlist, 1988; Wang et al, 2011a). More recently, the Immunological Genome Project has mapped the transcriptional profiles of multiple T cell populations and reported high levels of Myc mRNA in immune‐activated effector T cells (Best et al, 2013). However, the expression of Myc mRNA and protein can be quite discordant because of post‐transcriptional control of Myc protein (Vervoorts et al, 2006; Junttila & Westermarck, 2008; Thomas & Tansey, 2011; Ehninger et al, 2014). For example, stabilisation of Myc protein by a T58A mutation has been described in Burkitt's lymphoma (Yano et al, 1993; Gregory & Hann, 2000) and inactivating mutations of the E3 ubiquitin ligase Fbw7 that target Myc for proteasomal degradation are frequently found in T‐ALL (Welcker et al, 2004a; O'Neil et al, 2007).
The relevance of understanding the control of Myc protein levels in T cells was highlighted recently: immune‐activated T cells lacking the system L amino acid transporter Slc7a5 upregulate Myc mRNA but fail to express Myc protein and hence have global metabolic defects (Sinclair et al, 2013). In this context, many experiments have analysed Myc mRNA in T cells activated pharmacologically with phorbol esters, calcium ionophores and plant lectins (Kelly et al, 1983; Reed et al, 1987, 1988; Kelly & Siebenlist, 1988), but there is almost no detailed analysis of Myc protein in T cells responding to physiological stimuli. Accordingly, the present study has explored how engagement of the T cell antigen receptor (TCR) with peptide/major histocompatibility complexes (p/MHC) controls Myc expression. We have also examined how a key pro‐inflammatory cytokine interleukin‐2 (IL‐2) impacts on Myc expression. We show that the TCR is a digital switch that couples the strength of the antigen stimulus to the frequency of cells within a population that express Myc. However, TCR triggering alone cannot sustain expression of Myc and post‐transcriptional control of Myc protein by IL‐2, a γc cytokine that triggers Janus‐associated kinase (JAK)‐dependent signalling pathways, fine‐tunes Myc levels in individual T cells. We show that Myc is constantly phosphorylated by the serine/threonine kinase GSK3 in activated T cells and targeted for proteasomal degradation. Myc protein thus only accumulates in T cells with high levels of protein synthesis. This study also affords the insight that the cellular concentration of Myc matters in the context of T cell metabolism.
TCR signal strength determines Myc protein expression in a digital manner
The expression of Myc in T cells is controlled by the TCR (Wang et al, 2011a). A crucial question is how TCR signalling strength controls the pool size of T cells that differentiate to effector cells. In this respect, although Myc is required for T cell differentiation, the impact of antigen signalling strength on Myc expression has not been explored. To explore the sensitivity of Myc induction to different strengths of TCR ligand, we used the OT1 TCR transgenic model where there are well‐characterised peptide ligands with different affinities for the TCR (Daniels et al, 2006). These permit exploration of how the affinity of peptide‐major histocompatibility complexes (p/MHC), the physiological ligand for TCR complexes, dictates Myc expression. In these experiments, we activated OT1 T cells with TCR agonists of varying affinity: SIIQFEHL (Q4H7: Kd 51 ± 9.1 nM), SIITFEKL (T4: Kd of 55 ± 10.1 nM), SIIQFERL (Q4R7: Kd 48 ± 9.5 nM), SIIQFEKL (Q4: Kd 29 ± 7.2 nM) and SIINFEKL (N4: Kd 3.7 ± 0.7 nM) (Daniels et al, 2006). Western blot analysis of OT1 T cells shows that the level of Myc protein within a T cell population is determined by the strength of the TCR ligand (Fig 1A). Cellular levels of Myc mRNA are also determined by TCR ligand strength (Fig 1B), revealing that one fundamental way TCR agonists control Myc expression in T cells is by controlling the expression of Myc mRNA.
Changes in Myc levels in response to TCR ligand strength could reflect that ligand affinity governs the frequency of T cells within a population that express Myc. Alternatively, TCR ligand strength may dictate the amount of Myc expressed by each individual activated T cell. To distinguish these possibilities, we needed to directly visualise Myc protein expression at the single cell level. Accordingly, we used a mouse model in which a fusion protein of Myc and enhanced green fluorescent protein (GFP‐Myc) is expressed from the endogenous Myc locus (GFP‐MycKI) (Huang et al, 2008). We then used OT1 GFP‐MycKI T cells to assess whether the strength of the TCR ligand influenced the frequency of T cells expressing Myc within a population. Fig 1C shows the pattern of Myc expression in OT1 T cells activated with TCR agonists of varying affinity for the TCR. GFP‐Myc is not expressed in naïve CD8+ T cells but is rapidly induced following exposure to TCR peptide agonists (2 h). Following TCR engagement, two distinct cell populations were observed: a population with high GFP‐Myc expression and a population with no detectable Myc expression (Fig 1C, left panel). It was striking that the frequency of T cells that express Myc is determined by the strength of the TCR ligand (Fig 1C, middle panel). This on/off pattern of Myc expression suggested a bimodal/digital response pattern of Myc regulation. Consistent with a digital response, the mean fluorescence intensity (MFI) of Myc expression in the GFP‐Mycpos populations is not significantly different for the T4, Q4R7, Q4 or N4 peptides (Fig 1C, right panel). Hence, increasing the affinity of the TCR ligand does not increase the amount of Myc in individual responding cells. We also examined Myc expression following naïve OT1 T cell activation with increasing concentrations of the p/MHC ligand Q4. Fig 1D shows that the concentration of TCR ligand dictates the frequency of T cells that express Myc.
The bimodal, on/off pattern of Myc expression was also maintained during a sustained (20 h) T cell response to p/MHC ligands (Fig 1E). Here we compared the TCR ligand dose–response for induction of Myc and the activation marker CD69. Fig 1E (bottom panel) shows that the upregulation of CD69 is more sensitive to the TCR ligand dose than Myc induction (top panel). The expression of CD69 marks T cells that have responded to antigen, and in this respect, it was of note that Myc expression was restricted to the CD69‐expressing T cells and was bimodal in the CD69pos TCR‐activated lymphocytes (Fig 1F, left panel). We did however note that at this sustained time point, the level of p/MHC ligand not only directed the frequency of T cells that initiated Myc expression but also influenced the level of Myc per cell (Fig 1F, right panel).
One important question was whether the frequency of cells that expressed Myc protein in activated T cells was explained by differences in the frequency of T cells that express Myc mRNA. To answer this question, OT1 GFP‐MycKI T cells were activated with the N4 TCR agonist for 2 h before GFP‐Mycpos and GFP‐Mycneg T cells were purified by FACS and Myc mRNA was quantified. Fig 1G shows that N4‐stimulated GFP‐Mycpos OT1 T cells express high levels of Myc mRNA compared with GFP‐Mycneg OT1 T cells. This result is consistent with the hypothesis that the TCR controls the frequency of cells that express Myc because the TCR controls the frequency of cells that express Myc mRNA.
We next examined whether digital Myc expression is common to both CD4+ and CD8+ T cells. Fig 1H shows that GFP‐Myc is not expressed in naïve lymph node‐derived CD4+ and CD8+ T cells but is rapidly induced in both populations following polyclonal T cell activation with CD3 and CD28 antibodies with a clear digital response pattern of Myc regulation. In these experiments, we used saturating levels of CD3 antibodies, and within the first few hours of the activation response, there was an increase in the percentage of T cells that expressed Myc but no increase in the maximal amount of Myc expressed. Under these potent activation conditions, all T cells expressed Myc at the 24‐h time point. This response was sustained over a 72‐h period, but it was notable that the level of Myc per cell had decreased at the 48‐ and 72‐h time points (Fig 1H).
When T cells were activated polyclonally with different concentrations of CD3 antibody, then the frequency of Myc‐expressing cells directly correlated with the amount of CD3 antibody used (Fig 1I), and the digital nature of the response was preserved. In these experiments, the level of the costimulatory antibody CD28 was constant, indicating that it is the level of TCR engagement that determined Myc expression. The digital nature of Myc induction in response to TCR engagement is thus a common feature of the TCR response to both physiological and polyclonal ligands and occurs in both CD4+ and CD8+ T cells.
IL‐2/JAK signalling controls Myc expression in TCR‐activated T cells
The differentiation of antigen‐activated CD8+ T cells is regulated by γc cytokines such as interleukin‐2 (IL‐2). Antigen‐primed T cells cultured in IL‐2 thus differentiate to effector cytotoxic T cells (CTL) (Kalia et al, 2010; Pipkin et al, 2010). It has also been described that IL‐2 controls the expression of Myc (Reed et al, 1988; Lord et al, 2000). In this context, we observed that antigen receptor‐triggered T cells maintained in culture in the presence of receptor‐saturating levels of IL‐2 expressed high levels of Myc (Fig 2A). Moreover, it was striking that sustained IL‐2 signalling is required to maintain the high expression of Myc protein in CTL, with Myc levels decreasing within 1 h of withdrawal from IL‐2 (Fig 2B). We also examined the effect of two other γc cytokines, IL‐7 and IL‐15, on the expression of Myc in CTL. In this context, Myc expression is essential in vivo for signalling by IL‐15 (Bianchi et al, 2006; Dose et al, 2006, 2009; Mycko et al, 2009; Jiang et al, 2010). Fig 2C shows that IL‐2, IL‐15 and IL‐7 are different in their ability to maintain Myc protein expression in effector CTL. IL‐2 has the strongest effect, IL‐15 is much less potent at maintaining Myc expression, and there are only very low levels of Myc in effector CTL maintained in IL‐7.
IL‐2 and IL‐15 signal via a receptor complex that includes the common gamma chain (γc) and a β subunit (CD122). Triggering of this receptor complex activates the tyrosine kinases JAK1 and JAK3. IL‐2 is able to sustain a much higher level of signalling in activated T cells than IL‐15, even when both cytokines are at the receptor‐saturating concentrations (Cornish, 2006). The differential effect of IL‐2 and IL‐15 on Myc expression suggests that the level of JAK kinase activity might determine the expression of Myc. Recently, inhibitors of JAK kinases have been described, notably tofacitinib (Changelian et al, 2003). We could therefore test directly the contribution of JAK signalling to the regulation of Myc expression in IL‐2‐maintained CTL. Fig 2D shows that tofacitinib treatment leads to a rapid loss of Myc protein expression in IL‐2‐maintained CTL.
Immune‐activated T cells produce IL‐2 and can have autocrine responses to this cytokine (Feau et al, 2011; Sa et al, 2013). The ability of IL‐2 to control Myc expression in CTL made us question whether autocrine IL‐2/JAK signalling had any role in controlling Myc expression in TCR‐activated naïve T cells. We therefore examined the effect of the JAK inhibitor tofacitinib on Myc induction in TCR‐ and CD28‐activated T cells. Fig 2E shows that there was no effect of tofacitinib on Myc expression in T cells activated with CD3 and CD28 antibodies for 4 h, whereas there was a clear reduction in Myc expression in tofacitinib‐treated T cells at the 24‐ and 48‐h time point. It was notable that treatment of activated T cells with the JAK inhibitor did not change the frequency of activated T cells that express Myc but rather reduced the amount of Myc expression per cell. In further experiments, we examined the impact of PC61, a CD25 antibody that blocks IL‐2 binding to its high‐affinity receptor (Lowenthal et al, 1985), on Myc expression in T cells activated polyclonally with CD3 and CD28 antibodies. Fig 2F shows that blockade of IL‐2 binding to its receptor reduced Myc expression in the longterm‐activated T cells. However, the neutralising IL‐2 antibody had no impact on the digital TCR‐induced Myc response seen at 6 h. Inhibition of autocrine IL‐2 did not reduce the frequency of activated T cells that express Myc but could reduce Myc expression level per cell. Hence, IL‐2 control of Myc expression is an analogue response unlike the bimodal response pattern for TCR control of Myc expression.
The data above argue that there is no role for autocrine IL‐2/JAK signalling in the immediate response to TCR engagement, but during the sustained immune activation response, IL‐2 signalling does have an impact on Myc expression. In further experiments to explore this question, we took advantage of the fact that the level of IL‐2 signalling in a T cell is determined by the level of CD25 expression (Cantrell & Smith, 1984). Moreover, CD25 expression in T cells is controlled by a positive feedback mediated by JAK activation of the transcription factor STAT5 (Nakajima et al, 1997). If Myc expression in effector T cells is determined by the strength of IL‐2 signalling, then Myc levels will be highest in cells that express high levels of CD25. Fig 2G shows that the level of Myc protein in activated CD4+ and CD8+ T cells correlates with the expression of CD25. Similarly, when GFP‐MycKI mice are immunised with an attenuated strain of Listeria monocytogenes over 24 h, it is possible to identify immune‐activated CD25‐positive effector T cells (Fig 2H, left panels). These activated CD8+ T cells express Myc, whereas no Myc expression is detected in non‐responding naïve CD8+ T cells from the same animal (Fig 2H, right panel). Importantly, Myc expression levels in the activated CD8+ T cells correlate with the level of CD25 expression (Fig 2I). Collectively, these data are consistent with the hypothesis that IL‐2 activation of JAK signalling pathways controls cellular levels of Myc in effector T cells.
Transcriptional and post‐transcriptional control of Myc expression in T cells
T cell antigen receptor control of Myc expression was explained by TCR control of the frequency of cells that express Myc mRNA. IL‐2 regulates an analogue response that controls the amount of Myc expressed by each cell. We therefore assessed whether the analogue IL‐2 response reflected the control of Myc mRNA levels. Fig 2A shows that although there is a clear IL‐2 dose–response for Myc protein expression, there is no equivalent IL‐2 dose–response for Myc mRNA in CTL (Fig 3A). Similarly, the JAK inhibitor tofacitinib causes CTL to rapidly lose Myc protein but not Myc mRNA (Figs 2D and 3B). Moreover, CTL maintained in IL‐2, IL‐15 or IL‐7 have very different levels of Myc protein but express equivalent levels of Myc mRNA (Figs 2C and 3C). These data argue that the γc cytokines IL‐2 and IL‐15 primarily regulate Myc levels via post‐transcriptional mechanisms.
To rigorously test this model further, we transduced activated T cells with a FLAG‐MycWT‐IRES‐GFP retroviral construct (encoding a FLAG‐tagged wild‐type Myc cDNA and an IRES‐controlled GFP cDNA) and then cultured the cells in the presence or absence of IL‐2. CTL transduced with the Myc‐IRES‐GFP vector only overexpress ectopic Myc protein if the cells are cultured with IL‐2 (Fig 3D), whereas the IRES‐controlled GFP (Fig 3D) and Myc mRNA (Fig 3E) were detected in both the IL‐2‐maintained and IL‐2‐deprived T cells. These data show that in the absence of IL‐2, CTL cannot sustain the expression of Myc from endogenous or ectopically expressed retroviral Myc transcripts.
Myc protein has a short half‐life in T cells
One striking observation was the rapidity with which Myc protein was lost from CTL following IL‐2 withdrawal (Fig 2B). These data argue that Myc has a very short half‐life in activated T cells. One previously described mechanism to control the expression of Myc is a phosphorylation‐dependent pathway that targets Myc for proteasomal degradation (Gregory & Hann, 2000). Phosphorylation of Myc on T58 by glycogen synthase kinase 3β (GSK3β) promotes its interaction with Fbw7, the substrate recognition component of the SCFFbw7 ubiquitin ligase, and directs Myc ubiquitination and proteasomal degradation (Gregory et al, 2003; Welcker et al, 2004a,b). We have previously used high‐resolution mass spectrometry to map the phosphoproteome of IL‐2‐maintained CTL (Navarro et al, 2011). Analysis of this data revealed that Myc is phosphorylated on Ser62 and Thr58 in activated T cells (Fig 4A). In this respect, it has been described that the phosphorylation of Ser62 primes Myc for subsequent Thr58 phosphorylation by GSK3β (Sears et al, 1999, 2000). These data argue that Myc is constantly phosphorylated and targeted for degradation in IL‐2‐maintained CTL. To explore this hypothesis further, we examined the impact of MG132, a well‐characterised inhibitor of the 26S proteasome, on the expression of Myc in IL‐2‐maintained and IL‐2‐deprived CTL. These data show that MG132 promoted the expression of Myc in IL‐2‐maintained CTL and could also prevent the loss of Myc expression that normally accompanies IL‐2 withdrawal (Fig 4B). Moreover, if CTL were treated with the GSK3 inhibitor CHIR99021, they were able to sustain Myc expression following IL‐2 withdrawal (Fig 4C).
These data indicate that the short half‐life of Myc in T cells is controlled by GSK3β‐mediated phosphorylation of Myc Thr58, which then targets Myc for proteasomal degradation. This predicts that a Myc protein with the Thr58 mutated to a non‐phosphorylatable residue such as alanine would be expressed in T cells independent of the presence of γc cytokines. To test this hypothesis, we transduced antigen receptor‐activated T cells with a retroviral construct encoding MycT58A‐IRES‐eGFP and then cultured the cells in the presence or absence of IL‐2. The data show that MycT58A expression is sustained in CTL deprived of IL‐2 (Fig 4D). This is in marked contrast to the inability of IL‐2‐deprived T cells to sustain the expression of endogenous or ectopically expressed retroviral wild‐type Myc (Fig 3D).
The present results demonstrate that GSK3 constantly phosphorylates Myc on Thr58 in T cells and hence constantly targets Myc for degradation. Moreover, it was striking that the treatment of T cells with the proteasome inhibitor MG132 causes Myc to accumulate in IL‐2‐maintained CTL (Fig 4B). This demonstrates that there is a constant high rate of Myc proteolysis by the proteasome in IL‐2‐maintained T cells. Accordingly, Myc will only be able to accumulate in activated T cells when rates of Myc synthesis exceed the rates of Myc degradation. IL‐2 is very potent at inducing amino acid uptake and protein synthesis in CTL (Cornish, 2006; Sinclair et al, 2013). High rates of amino acid uptake and consequently high rates of protein synthesis in IL‐2‐maintained CTL could therefore explain why Myc accumulates in IL‐2‐maintained CTL and could also explain why IL‐15 is unable to sustain high levels of Myc in CTL: IL‐15 is much less potent than IL‐2 in its ability to promote protein synthesis (Fig 5A).
Recently, we have shown that expression of system L amino acid transporter Slc7a5 by TCR‐activated cells is essential for the expression of Myc protein (Sinclair et al, 2013). IL‐2 can sustain high levels of Slc7a5 expression and CD98, the two subunits of the system L amino acid transporter (Fig 5B), and system L‐mediated amino acid transport in CTL (Fig 5C). In contrast, IL‐15 is much less potent at inducing Slc7a5 and CD98 expression (Fig 5B) and IL‐15‐maintained cells exhibit much lower rates of system L amino acid transport (Fig 5C). We considered whether the ability of the JAK inhibitor tofacitinib to decrease Myc expression in T cells could be caused by a requirement of JAK activity for system L amino acid uptake and protein synthesis in activated T cells. Fig 5D addresses this question and reveals a striking reduction of system L transport activity and very low rates of protein synthesis in CTL treated with tofacitinib.
These results collectively argue that T cells need continual high rates of amino acid uptake to sustain high levels of Myc protein. To test this hypothesis directly, we looked at the impact of amino acid deprivation on Myc expression in activated T cells; indeed, amino acid deprivation caused IL‐2‐maintained CTL to rapidly lose the expression of Myc (Fig 5E). Additionally, blockade of system L transport by the inhibitor 2‐amino‐2‐norbornanecarboxylic acid (BCH) also prevented the upregulation of Myc protein in activated CD8+ T cells (Fig 5F). Moreover, TCR‐stimulated GFP‐Mycpos OT1 T cells have high levels of Slc7a5 and CD98 mRNA compared to GFP‐Mycneg OT1 T cells (Fig 5G). Thus, Myc protein levels in immune‐activated T cells are matched to high expression of amino acid transporters and to high rates of amino acid uptake. One consideration in these experiments is that inhibition of amino acid transport will cause loss of mTORC1 activity (Sinclair et al, 2013). However, we have shown previously that inhibition of mTORC1 does not prevent Myc expression in TCR‐ or IL‐2‐activated CD8+ T cells (Finlay et al, 2012; Sinclair et al, 2013).
Myc levels are important for activated T cells
The mechanisms whereby TCR signalling strength controls the pool size of T cells that differentiate to effector cells are not fully understood. In the absence of Myc, T cells cannot respond to TCR triggering to proliferate or differentiate to effector cells (Wang et al, 2011b). The present data now show that when GFP‐MycKI OT1 T cells are activated with p/MHC ligands, it is the GFP‐Mycpos cells that express the effector cytokine interferon gamma (IFNγ) mRNA, whereas GFP‐Mycneg cells from the same cultures do not (Fig 6A). Moreover, in the sustained responses to p/MHC ligands, it is the GFP‐Myc‐expressing OT1 T cells that produce high levels of IFNγ and not the GFP‐Mycneg T cells (Fig 6B). We also observed that the level of IFNγ in an individual cell correlates with the level of expression of GFP‐Myc (Fig 6C).
T cell antigen receptor engagement triggers a growth response in T cells causing them to increase in cell size (blastogenesis) as judged by flow cytometric analysis of the forward and side scatter properties of activated T cells. We thus used flow cytometry to analyse the forward and side scatter properties of GFP‐MycKI OT1 T cells activated with the p/MHC ligands Q4 and T4. The expression of Myc in the CD69+ TCR‐activated cells had a bimodal response as described in Fig 1. Fig 6D shows that it is the GFP‐Myc‐expressing cells that have undergone blastogenesis. We also analysed blastogenesis of GFP‐MycKI T cell populations activated polyclonally with CD3 and CD28 antibodies. As described above, when T cells are activated polyclonally with different concentrations of CD3 antibody, then the frequency of Myc‐expressing cells directly correlated with the dose of TCR ligand used. Fig 6E shows GFP‐Myc and CD69 expression in CD8+ T cells stimulated with a low concentration of the CD3 antibody. A large percentage of the cells responded to TCR ligation to induce CD69 expression, but only a subset of the CD69+ cells express GFP‐Myc; that is, Myc induction is bimodal in the TCR‐activated CD69+ T cells. Fig 6F shows that CD69+ CD8+ T cells that do not express Myc have increased cell size in comparison with the CD69− quiescent CD8 T cells. However, the Myc‐expressing CD69+ CD8+ T cells are much larger than the Myc‐negative CD69+ CD8+ T cells. Importantly, T cells with both Myc alleles deleted do not blast in response to TCR and CD28 activation (Fig 6G).
How important is it that the amount of Myc protein expressed in a single, activated T cell can be fine‐tuned? Strategies to address this issue require the ability to quantitatively analyse a Myc‐regulated response in single T cells. In this regard, there is strong evidence that Myc regulates transferrin receptor expression (O'Donnell et al, 2006) (Holland et al, 2012). Moreover, there are good tools for single cell analysis of this pathway that would allow a direct analysis of the importance of Myc protein levels for transferrin uptake. We first addressed whether Myc was indeed important for transferrin receptor expression in T cells. Naïve T cells do not express the transferrin receptor (CD71), but expression of this receptor, and the cellular uptake of transferrin, is strongly induced in antigen receptor‐activated T cells (Fig 7A). T cells with both Myc alleles deleted cannot upregulate CD71 or transferrin uptake in response to TCR engagement (Fig 7B). Is the level of Myc expression per cell important for transferrin receptor expression? To explore this, we first used the GFP‐MycKI mouse model and examined CD71 expression versus GFP‐Myc expression in TCR‐activated CD4+ and CD8+ T cells. The data show a clear correlation between expression of CD71 and Myc (Fig 7C).
There was also a strong correlation between cellular levels of Myc and expression of transferrin receptors in CTL cultured in the cytokines IL‐2 and IL‐15. Fig 7D thus shows that IL‐2‐maintained CTL express high levels of CD71 and uptake high amounts of transferrin compared to T cells deprived of cytokines, with expression of CD71 and transferrin uptake in activated T cells cultured in IL‐15 being intermediate. This correlates with the ability of IL‐2 to maintain high levels of Myc protein compared to IL‐15 (Fig 2C). These data are correlative; hence, to test whether differences in Myc expression levels were causal for differences in CD71 expression, we examined the impact of increasing Myc levels in T cells cultured under these different conditions. In these experiments, we looked at the impact of expressing the MycT58A mutant on CD71 expression and transferrin uptake because the use of this mutant bypasses the GSK3‐mediated pathway that rapidly targets Myc for degradation and allows overexpression of Myc even when cells are cytokine‐deprived. In this respect, Fig 7E shows that GSK3 inhibition using CHIR99021, which prevents Myc degradation, could increase CD71 expression in IL‐2‐maintained CTL. There was also a strong effect of MycT58A expression on CD71 expression and the ability of cells to take up transferrin in cytokine‐maintained CTL. Hence, ectopic expression of MycT58A increased expression of CD71 and transferrin uptake in both IL‐15‐ and even IL‐2‐cultured CTL (Fig 7F). Ectopic expression of MycT58A was also able to sustain expression of CD71 and transferrin uptake in IL‐2‐deprived CTL. In addition, increasing Myc levels increased transferrin uptake in IL‐15‐cultured CTL to the level seen in the control IL‐2‐maintained cells. Hence, the limiting factor for transferrin receptor expression and transferrin uptake in IL‐15‐maintained CTL was the level of Myc expression. Moreover, the fact that expression of MycT58A, which increased cellular concentrations of Myc, increases rates of transferrin uptake in IL‐2‐maintained cells (Fig 7G) shows that the concentration of Myc levels per cell dictates transferrin receptor expression and rates of transferrin uptake by immune‐activated T cells. There is thus a clear biological consequence of fine‐tuning Myc expression in single, activated T cells.
The expression of Myc in CD8+ T cells is regulated by both antigen receptor signals and the γc cytokine IL‐2. The present study now shows that the TCR and IL‐2 use distinct mechanisms to control Myc levels in T cells. The TCR controls Myc expression in a digital response that determines the frequency of the T cell population that switches on Myc mRNA and protein expression. In contrast, the cytokine IL‐2 regulates Myc expression in an analogue response that fine‐tunes Myc protein levels per cell. In the immediate response to TCR engagement, the strength of TCR signal controls how many cells express Myc, and at these time points there is no apparent role for IL‐2/JAK signalling. Myc expression in T cells thus appears to be a two‐stage process; Myc expression is digitally induced by the strength of TCR signalling, but the maintenance of high Myc expression then becomes dependent upon other external stimuli such as IL‐2. Myc is essential for the metabolic reprogramming that controls effector T cell differentiation (Wang et al, 2011a). The fact that the strength of the TCR ligand determines the frequency of T cells that express Myc gives new insight about the mechanisms that allow TCR signalling strength to control the pool size of T cells that metabolically reprogramme and differentiate to effector cells.
One striking observation from the present study was the discordance between Myc protein and mRNA levels in immune‐activated T cells. This latter observation is relevant because many previous studies have interrogated Myc mRNA expression in T lymphocyte subpopulations (Best et al, 2013). The data herein show that T cells can express high levels of Myc RNA but that high levels of Myc protein can only be sustained in T cells that have high rates of amino acid uptake. Myc expression in an antigen receptor‐stimulated T cell will thus be transient unless the T cell can sustain high rates of biosynthesis of Myc protein. A key mechanism that controls Myc protein expression in activated T cells is mediated by the serine/threonine kinase GSK3. Hence, in activated T cells Myc is phosphorylated by GSK3 on Thr58, which then constantly targets the protein for proteasomal degradation (Gregory et al, 2003). It is this constant high rate of Myc degradation in activated T cells that confines high levels of Myc protein expression to T cells with high rates of amino acid uptake and protein synthesis. Myc protein expression thus rapidly declines in situations where T cell protein synthesis and amino acid uptake are limited. Recent studies have shown that there is very tight control of amino acid transport and hence protein synthetic capacity during the immune activation of T cells (Hayashi et al, 2013; Sinclair et al, 2013). The critical signals that are known to be able to induce and sustain high‐level expression of amino acid transporters in T cells are antigen and pro‐inflammatory cytokines such as IL‐2 (Wang et al, 2011a; Sinclair et al, 2013). This means that Myc protein expression will be restricted to T cells responding to immune activation or to T cells exposed to pro‐inflammatory cytokines that can maintain amino acid uptake.
One of the cytokines that can sustain high levels of Myc protein in T cells is IL‐2. This molecule is a member of the γc family of cytokines that signal by activating the JAK tyrosine kinases. The present experiments interrogated the role of JAKs regulating Myc expression using the JAK inhibitor tofacitinib: a drug showing clinical promise for the treatment of autoimmune diseases (Hsu & Armstrong, 2014; Lee et al, 2014). Our data afford the insight that immune‐activated T cells can express high levels of Myc mRNA and yet be dependent on sustained JAK activity to express Myc protein. Moreover, another novel insight from the present experiments is that part of the tofacitinib mechanism of action as an immunosuppressant may be to prevent T cell reprogramming of Myc‐controlled metabolic responses. In the context of γc cytokines and JAKs, the strength of IL‐2 signalling during an immune response determines effector versus memory cell fate of immune‐activated CD8+ T cells (Kalia et al, 2010). Herein we show that IL‐2 has the ability to sustain high rates of Myc expression compared to other γc cytokines such as IL‐7 and IL‐15, and this could contribute to the unique role for this cytokine as a regulator of peripheral T cell metabolism and differentiation. What is the mechanistic explanation for the differential effect of IL‐2, IL‐7 and IL‐15? They all signal through the γc, and IL‐2 and IL‐15 share the same beta receptor subunit. Recent studies have shown that it is predominantly the abundance of the specific alpha chain for IL‐2 and IL‐15 that determines the strength of signal mediated by that cytokine (Ring et al, 2012). Furthermore, in T cells that highly express CD25, the alpha subunit for the high‐affinity IL‐2 receptor, signalling through IL‐15 and IL‐7 in particular is attenuated because of the sequestration of γc subunits in complete IL‐2 receptors (Cotari et al, 2013). Therefore, even at saturating concentrations, IL‐7 and IL‐15 are less potent than IL‐2 in our system.
The ability of T cells to rapidly fine‐tune intracellular concentrations of Myc is striking but is it important? How sensitive are T cells to changes in Myc protein levels? We addressed this question by interrogating the importance of Myc protein levels for transferrin uptake. We show that Myc is essential for transferrin receptor expression in immune‐activated T cells. Moreover, a salient result was that Myc protein levels determine the level of transferrin receptor expression and rates of transferrin uptake by immune‐activated T cells. Myc is thus not an on/off switch for transferrin receptor expression but can fine‐tune expression of this key receptor that ensures that T cells have sufficient iron. Myc has other roles in T cells, for example to control glucose and glutamine metabolism and to regulate expression of key transcription factors such as AP4 (Wang et al, 2011a; Chou et al, 2014). The present observation that there is coordination of Myc protein expression with amino acid uptake thus reveals a mechanism that would ensure that T cells coordinate increases in glucose and glutamine and iron metabolism to match the biosynthetic demands associated with the immune activation of T cells.
Materials and Methods
Mice and cell culture
All mice were kept in the Biological Resource Unit at the Wellcome Trust Biocentre, University of Dundee, in accordance with UK Home Office (Animals) Scientific Procedures Act 1986. Mice used were OT1 TCR transgenic mice, which express a TCR recognising the ovalbumin (OVA)‐derived peptide SIINFEKL, or P14 TCR transgenic mice, which express a TCR recognising the gp33‐41 peptide of LCMV (KAVYNFATM). GFP‐MycKI was used as described (Huang et al, 2008). CD4Cre+ x Mycfl/fl and control CD4Cre− x Mycfl/fl were used as previously described (Mycko et al, 2009). All mice are on a C57BL/6 genetic background and were used between 12 and 24 weeks of age.
For experiments involving T cell receptor (TCR) stimulation, CD3 antibody (2C11, 0.5 μg/ml) and CD28 antibody (clone 37.51, eBioscience, 3 μg/ml) were used for polyclonal T cell activation whilst OVA‐derived peptides (10 ng/ml unless otherwise stated) were used for OT1 T cell activation for the specified times.
For experiments using cytotoxic T lymphocytes (CTL), cells were generated as described in Waugh et al (2009). Briefly, splenic CD8+ T cells from P14 mice were activated with 100 ng/ml gp33‐41 peptide, washed and maintained with 20 ng/ml IL‐2 (Novartis) or IL‐15 (Peprotech) for a further 3–5 days, or in IL‐7 (5 ng/ml, Peprotech) as indicated. Culture medium consisted of RPMI 1,640 medium containing L‐glutamine (Invitrogen) with 10% heat‐inactivated foetal calf serum (Gibco), penicillin–streptomycin (Gibco) and 50 μM β‐mercaptoethanol (Sigma).
The proteasome inhibitor MG132 and GSK3 inhibitor CHIR99021 were synthesised by DSTT, University of Dundee. Tofacitinib (GSK) was used at 100 nM unless otherwise stated. Anti‐mouse CD25 antibody (eBioscience, clone PC61.5) and IgG1 isotype control (eBioscience, clone eBRG1) were used at 2 μg/ml. For experiments involving T cell culture with the system L blocker 2‐amino‐2‐norbornanecarboxylic acid (BCH, Sigma), cells were cultured in 50% RPMI culture medium and 50% Hanks' buffered saline solution with or without 50 mΜ BCH.
An attenuated Act‐A‐deleted strain of Listeria monocytogenes that expresses OVA was used courtesy of Professor Hao Shen (Pearce & Shen, 2007). GFP‐MycKI and WT control mice were immunised by intravenous injection of 5 × 106 colony‐forming units. Mice were culled after 24 h and spleens harvested for analysis.
The GFP control plasmid construct was made by PCR amplification of EGFP from a pEGFP construct (Clontech) and cloning into the pBMN‐LZRS vector (Addgene) as a HindIII/NotI fragment, replacing the lacZ gene. MycT58A cDNA was generated by in vitro mutagenesis and the mutation confirmed by sequencing before cloning into the pBMN‐I‐GFP vector as an EcoRI fragment. Phoenix ecotropic packaging cells (Swift et al, 2001) were used to generate virus. The retroviral infection protocol of T cells was performed as previously described (Waugh et al, 2009).
Flow cytometry and cell sorting
The following fluorochrome‐conjugated antibodies (BD Pharmingen or eBioscience) were used for staining: CD4 (RM4‐5), CD8 (53‐6.7), TCRβ (H57‐597), CD25 (PC61), CD44 (IM7), CD69 (H1.2F3), CD71 (C2F2), CD98 (RL388), IFNγ (XMG1.2), anti‐GFP (rabbit polyclonal, Life technologies, for fixed samples in Listeria immunisation experiments) and Fc Block (2.4G2). DAPI was used as a live/dead discriminator.
Data were collected on FACSCalibur, Verse and LSR Fortessa machines (Becton Dickinson) and analysed using FlowJo software (Treestar). Fluorescence‐activated cell sorting (FACS) was performed on a FACSVantage Cell Sorter (Becton Dickinson) to separate CD8+ GFP‐Mycpos and CD8+ GFP‐Mycneg live cell populations.
Transferrin uptake assay
Cells were resuspended at 5 × 105/ml in RPMI 5% BSA for 2 h prior to assay and then washed with RPMI 0.5% BSA before incubation with transferrin‐alexa647 conjugate (Sigma, 5 μg/ml) at 37°C for 5 minutes. Uptake was stopped by washing twice with ice‐cold acid wash (150 mM NaCl, 20 mM citric acid, pH 5.0). Transferrin uptake was measured by flow cytometry.
Amino acid uptake
CTL were re‐suspended in methionine‐free RPMI 1640 (Gibco Invitrogen) at 1 × 106/ml. Triplicate samples were incubated in 96‐well plates for 15 min before addition of 3H methionine (Perkin Elmer, 5 μCi/ml) and harvested after 15‐min incubation at 37°C onto glass fibre plates (Perkin Elmer). Plates were soaked in HiSafe scintillant (Perkin Elmer) and incorporated 3H counted using a 1450 microβ+ counter (Wallac).
CD8+ T cells were negatively selected from lymph nodes using AutoMacs (Miltenyi Biotechnology) prior to mRNA extraction. RNA was extracted from CTL or naïve cells using the RNeasy Minikit (Qiagen) and used to make cDNA using the cDNA synthesis kit (Quanta Biosciences). Quantitative real‐time PCR (qPCR) was performed on an iQ5 (Bio‐Rad) using SYBR Green Fastmix (Quanta Biosciences). The primers used are listed in Supplementary Methods.
TCR‐stimulated CD8+ T cells were purified by AutoMacs (Miltenyi Biotechnology) prior to protein extraction. Standard Western blotting protocols as described in Waugh et al (2009) were used. Blots were probed with antibodies recognising Myc, ERK1/2, pY694 STAT5, pan STAT5, GSK3α/β (Cell Signalling Technology), SMC1 (Cambridge Bioscience) and GFP (Roche Life Science). Densitometric analysis was performed using ImageJ software.
Data sets were analysed using SigmaPlot v11.0 (Systat Software Inc., USA) or Prism 6. Comparisons between two groups were made using Student's t‐test or a non‐parametric Wilcoxon rank‐sum test where appropriate. Comparisons between multiple groups were made using one‐way analysis of variance (ANOVA) test. Levels of significance are denoted as follows: * P < 0.05, ** P < 0.01, *** P < 0.001. Non‐significant results are either not marked or indicated ns.
GCP, AK and LVS performed most of the experiments. MNN performed in vivo Listeria immunisation. JLH analysed mass spectrometry data. IF and HRM provided critical reagents and advice. GCP, LVS, VHC and DAC were involved in conceptual design and manuscript authorship.
Conflict of interest
The authors declare that they have no conflict of interest.
Supplementary Materials and Methods
The authors thank the Division of Signal Transduction and Therapeutics (DSTT) and Elizabeth Emslie for making plasmid constructs; Dr. Rosie Clarke and Miss Arlene Whigham for fluorescence‐activated cell sorting; members of the Biological Services Resource Unit for animal care; Dr. Julia Kristensson for advice on in vivo experiments; and members of the Cantrell laboratory for critical evaluation of the manuscript. This work was funded by a Wellcome Trust Principal Research Fellowship (D.A.C.), Program Grant nos. 065975/Z/01/A and 097418/Z/11Z, and Tenovus Scotland.
FundingWellcome Trust Principal Research Fellowship065975/Z/01/A097418/Z/11Z
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