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The Journal of Immunology, 2001, 167: 2074-2080.
Copyright © 2001 by The American Association of Immunologists

Adenosine 3',5'-Cyclic Monophosphate (cAMP)-Dependent Inhibition of IL-5 from Human T Lymphocytes Is Not Mediated by the cAMP-Dependent Protein Kinase A1

Karl J. Staples*, Martin Bergmann2,*, Katsuyuki Tomita*, Miles D. Houslay{dagger}, Ian McPhee{dagger}, Peter J. Barnes*, Mark A. Giembycz* and Robert Newton3,*

* Department of Thoracic Medicine, National Heart and Lung Institute, Imperial College School of Medicine, London, United Kingdom; and {dagger} Division of Biochemistry and Molecular Biology, University of Glasgow, Glasgow, United Kingdom.


   Abstract
Top
 Abstract
Introduction
 Materials and Methods
 Results
 Discussion
 References
 
IL-5 is implicated in the pathogenesis of asthma and is predominantly released from T lymphocytes of the Th2 phenotype. In anti-CD3 plus anti-CD28-stimulated PBMC, albuterol, isoproterenol, rolipram, PGE2, forskolin, cholera toxin, and the cAMP analog, 8-bromoadenosine cAMP (8-Br-cAMP) all inhibited the release of IL-5 and lymphocyte proliferation. Although all of the above compounds share the ability to increase intracellular cAMP levels and activate protein kinase (PK) A, the PKA inhibitor H-89 failed to ablate the inhibition of IL-5 production mediated by 8-Br-cAMP, rolipram, forskolin, or PGE2. Similarly, H-89 had no effect on the cAMP-mediated inhibition of lymphocyte proliferation. Significantly, these observations occurred at a concentration of H-89 (3 µM) that inhibited both PKA activity and CREB phosphorylation in intact cells. Additional studies showed that the PKA inhibitors H-8, 8-(4-chlorophenylthio) adenosine-3',5'-cyclic monophosphorothioate Rp isomer, and a myristolated PKA inhibitor peptide also failed to block the 8-Br-cAMP-mediated inhibition of IL-5 release from PBMC. Likewise, a role for PKG was considered unlikely because both activators and inhibitors of this enzyme had no effect on IL-5 release. Western blotting identified Rap1, a downstream target of the cAMP-binding proteins, exchange protein directly activated by cAMP/cAMP-guanine nucleotide exchange factors 1 and 2, in PBMC. However, Rap1 activation assays revealed that this pathway is also unlikely to be involved in the cAMP-mediated inhibition of IL-5. Taken together, these results indicate that cAMP-elevating agents inhibit IL-5 release from PBMC by a novel cAMP-dependent mechanism that does not involve the activation of PKA.


   Introduction
Top
 Abstract
 Introduction
Materials and Methods
 Results
 Discussion
 References
 
Asthma is a complex inflammatory disease characterized by eosinophil infiltration into the airways (1). IL-5 is thought to be a major cytokine involved in this eosinophilia (2) and is an important regulator of eosinophil differentiation, maturation, and survival (3, 4). Although IL-5 is produced by eosinophils, mast cells, and epithelial cells (5, 6, 7), it is T cells of the Th2 phenotype that are the major source (8, 9).

The most common therapy for acute asthmatic bronchospasm are {beta}2-adrenoceptor agonists, which elevate intracellular cAMP and promote smooth muscle relaxation (10). However, cAMP may also inhibit inflammatory cell proliferation and the release of proinflammatory cytokines (11, 12, 13). These properties have led to the proposal that cAMP-elevating drugs such as phosphodiesterase (PDE)4 inhibitors may also show anti-inflammatory potential in the treatment of inflammatory diseases such as asthma and chronic obstructive pulmonary disease (14, 15).

Classically, cAMP exerts its effects by activating the cAMP-dependent protein kinase (PK), PKA, which subsequently phosphorylates downstream effector proteins such as myosin L chain kinase and CREB (16, 17, 18, 19, 20). However, the role of PKA in the anti-inflammatory effects of cAMP is less well established. Furthermore, alternative mechanisms of cAMP action that involve cAMP binding to and activating small guanine nucleotide exchange factors (GEFs) have been described (21, 22). One such GEF, known as exchange protein directly activated by cAMP (Epac) can, when bound by cAMP, directly activate the small Ras-like GTPase Rap1 to elicit downstream responses (21).

We have recently shown inhibition of IL-5 release and mRNA by cAMP-elevating agents in PBMC (23). In the present study, we have used the T cell-specific stimuli anti-CD3 plus anti-CD28 to evoke a T cell-specific response, allowing us to examine the mechanism by which cAMP inhibits IL-5 release from T cells.


   Materials and Methods
Top
 Abstract
 Introduction
 Materials and Methods
Results
 Discussion
 References
 
Reagents

Anti-CD3 (UCHT1) and anti-CD28 (CD28.2) Abs were purchased from BD PharMingen (Cambridge, U.K.). PGE2, 8-bromoadenosine cAMP (8-Br-cAMP), cholera toxin (CTX), and forskolin were obtained from Sigma (Poole, U.K.). Rolipram was obtained from Schering-Plough (Berlin, Germany). PD098059, SB203580, H-8, H-89, and a myristolated PKA inhibitor peptide (PKI) were purchased from Calbiochem (Nottingham, U.K.). 8-(4-chlorophenylthio) adenosine-3',5'-cyclic monophosphorothioate Rp isomer (Rp-8-CPT-cAMP), {beta}-phenyl-1, N2-etheno-8-bromoguanosine-3',5'- cyclic monophosphorothioate Sp isomer (Sp-8-Br-PET-cGMPS), and 8-(4-chlorophenylthio)guanosine-3',5'-cyclic monophosphorothioate Rp isomer (Rp-8-pCPT-cGMPS) were obtained from Biolog Life Science Institute (Bremen, Germany).

Preparation and treatment of human PBMC

Mononuclear cells were prepared from peripheral blood of healthy human volunteers and cultured at a density of 3 x 106 cells/ml for all experiments, as previously described (23). Cells were stimulated by the addition of anti-CD3 (UCHT1) and anti-CD28 (CD28.2) Abs, each at 500 ng/ml in solution, as previously described (23).

IL-5 ELISA

Supernatants from 3 x 106 cells were harvested 24 h after treatment, and ELISA was performed as described by the manufacturer (BD PharMingen). Human rIL-5 (R&D Systems, Minneapolis, MN) was used as a standard.

FACS analysis of proliferation

The proliferation assay was adapted from the method of Lu and Lane (24). PBMC (6 x 106 cells/treatment) were cultured for 44 h in the presence or absence of treatments as indicated, and then 50 µM 5-bromo-2'-deoxyuridine (BrdU) (Sigma) was added for a further 4 h. After harvesting, cells were washed with ice-cold PBS and fixed in cold 70% (v/v) ethanol overnight at -20°C. Cells were washed with ice-cold PBS and incubated for 30 min at room temperature in 2 M HCl and 0.5% (v/v) Triton X-100. Cells were washed once with 0.1 M sodium tetraborate before washing with PBS, 0.5% (v/v) Tween 20, and 1% (w/v) BSA. Cells were then incubated for 30 min at room temperature with a mouse anti-BrdU Ab (Amersham Pharmacia Biotech, Piscataway, NJ). After washing, cells were incubated with FITC-labeled anti-mouse Ab (DAKO, Ely, U.K.) for 30 min at room temperature. After further washing, cells were resuspended in PBS, 200 µg/ml RNase A, and 50 µg/ml propidium iodide. Flow cytometric analysis (BD Biosciences, Oxford, U.K.) and gating of proliferating cells was performed as previously described (24).

PKA assays

PBMC (12 x 106 cells/treatment) were harvested after 1 h, washed with HBSS, and assayed according to the method described by Giembycz and Diamond (25).

Rap1 activation assays

PBMC (24 x 106 cells/treatment) were harvested after 30 min, washed with HBSS, and assayed as described previously (26, 27).

Western blotting

PBMC (24 x 106 cells/treatment) were washed with HBSS and lysed on ice in 10 mM HEPES (pH 7.9), 1.5 mM MgCl2, 10 mM KCl, 0.5 mM DTT, and 0.1% (v/v) Nonidet P-40 supplemented with proteinase inhibitors. Total proteins (20 µg) were run on 10% SDS-PAGE and electroblotted onto nitrocellulose membranes (Amersham Pharmacia Biotech). Immunodetection of pan-CREB and phospho-CREB (New England Biolabs, Hitchin, Herts, U.K.) and Rap1 (Transduction Laboratories, Lexington, KY) was conducted according to the manufacturer’s instructions.

Statistical analysis

Analyses were performed using Kruskal-Wallis or Friedman ANOVA or Wilcoxon’s signed rank test as appropriate. Results were considered significant if p < 0.05 (***, p < 0.001; **, p < 0.01; and *, p < 0.05).


   Results
Top
 Abstract
 Introduction
 Materials and Methods
 Results
Discussion
 References
 
Inhibition of IL-5 production by cAMP-elevating drugs

We have previously shown that costimulation of PBMC for 24 h with activating Abs directed to the CD3 and CD28 surface markers is a T cell-specific stimulus that produced measurable quantities of IL-5 (23). This IL-5 release was profoundly inhibited by the cAMP analog 8-Br-cAMP, the PDE4 inhibitor rolipram, the Gs activator CTX, the adenylate cyclase activator forskolin, as well as by PGE2 (Fig. 1GoA). In addition, the {beta}2-adrenoceptor agonists albuterol and isoproterenol also inhibited IL-5 release (Fig. 1GoB). Furthermore, dose dependence was shown for 8-Br-cAMP, rolipram, forskolin, and PGE2 (Fig. 2GoA). These effects occurred at EC50 values within the range expected for either stimulation of adenylate cyclase or inhibition of PDE4, as appropriate.



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  		FIGURE 1. cAMP-elevating agents inhibit IL-5 production. A, Cells were incubated with anti-CD3 (500 ng/ml) plus anti-CD28 (500 ng/ml) and coincubated with rolipram (30 µM), 8-Br-cAMP (1 mM), CTX (2 µg/ml), PGE2 (1 µM), and forskolin (1 µM). After 24 h, supernatants were harvested for IL-5 determination. Data are expressed as picograms per milliliter and are plotted as means ± SEM (rolipram, n = 9; 8-Br-cAMP, n = 7; CTX, n = 9; PGE2, n = 9; and forskolin, n = 7). Significance was assessed using ANOVA (Kruskal-Wallis) with a Dunn’s post-test. B, Cells were stimulated as in A, described above, and treated with either albuterol or isoproterenol (1 µM) before IL-5 determination after 24 h. Data are expressed as a percentage of anti-CD3 plus anti-CD28-stimulated cells and are plotted as means ± SEM (albuterol, n = 11; and isoproterenol, n = 10). Significance was assessed using the Wilcoxon’s signed rank test. C, Cells were incubated with anti-CD3 and anti-CD28 as described above and coincubated with various concentrations of forskolin in the absence ({blacksquare}) or presence ({blacktriangledown}) of rolipram (10 nM) as indicated. Supernatants were harvested at 24 h for IL-5 determination. Data are expressed as a percentage of anti-CD3 plus anti-CD28-stimulated cells and are plotted as means ± SEM (n = 3).

 


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  		FIGURE 2. Effect of PK inhibitors on the inhibition of IL-5 by cAMP-elevating drugs. A, PBMC were incubated with anti-CD3 plus anti-CD28 as described above and coincubated with various concentrations of PGE2, rolipram, 8-Br-cAMP, and forskolin with or without H-89 (3 µM). Supernatants were harvested at 24 h, and IL-5 release measured. Data are expressed as means ± SEM of three independent experiments ({blacksquare}, without H-89; and {blacktriangledown}, with H-89). B, PBMC were stimulated with anti-CD3 plus anti-CD28 as described above or with 8-Br-cAMP (1 mM) and coincubated with or without Rp-8-pCPT-cGMPS (30 or 300 µM). Supernatants were harvested at 24 h, and IL-5 release measured. Data are expressed as means ± SEM of five independent experiments.

 
For many cAMP-dependent responses, particularly in regard to control of smooth muscle tone, simultaneous treatment with compounds that activate adenylate cyclase and inhibit PDE is predicted to result in a greatly enhanced level of cAMP to and lead to enhanced cAMP-dependent responses (28, 29). To test the relationship between activation of adenylate cyclase and PDE inhibition, cells were stimulated with anti-CD3 plus anti-CD28, and the effect of various concentrations of forskolin in the presence of rolipram was analyzed (Fig. 1GoC). Forskolin dose-dependently inhibited release of IL-5 (IC50 = 0.95 µM) and, in the presence of rolipram (10 nM), which alone caused a ~30% inhibition of IL-5 release, there was no obvious change in the concentration-response relationship to forskolin (EC50 = 0.64 µM). These data suggest that inhibition of IL-5 release by forskolin and rolipram may be by distinct pathways and not via a common cAMP pool.

Effect of kinase inhibitors

Pretreatment of PBMC with 3 µM H-89 had no effect on the inhibition of anti-CD3 plus anti-CD28-induced IL-5 generation by 8-Br-cAMP, rolipram, PGE2, or forskolin (Fig. 2GoA). Similarly, a less selective PKA inhibitor, H-8 (3 µM) (30), the cAMP antagonist Rp-8-CPT-cAMP (10 µM), which blocks the cAMP binding site of the inhibitory subunit of PKA but does not cause dissociation of the active enzyme (31), and a myristolated PKI (10 µM) (32) all had no effect on the 1 mM 8-Br-cAMP-induced inhibition of IL-5 release (data not shown).

Because T cells express PKG and this can be activated by cAMP, the possibility of PKG-mediated effects were tested (33, 34). Cells stimulated with anti-CD3 plus anti-CD28 were incubated with 8-Br-cAMP in the presence of the PKG inhibitor Rp-8-pCPT-cGMPS (30 or 300 µM). However, no reversal of the cAMP-mediated inhibition of IL-5 was observed (Fig. 2GoB). Similarly, stimulation with anti-CD3 plus anti-CD28 and coincubation with the active cGMP analog Sp-8-Br-PET-cGMPS (300 µM) had no effect on IL-5 release (data not shown). As cGMP analogs have been shown to penetrate T cells and demonstrate biological activity, these data suggest that PKG does not mediate the repression of IL-5 observed in this study (34).

A number of reports have suggested that mitogen-activated protein kinases (MAPKs) may mediate some of the responses to cAMP. The selective MAPK kinase 1 (MKK1) inhibitor PD098059 and the p38 MAPK inhibitor SB203580, which show IC50 values of 2–7 and 0.6 µM, respectively, were therefore tested (35, 36). In each case, drug concentrations of 10 and 3 µM, respectively, were selected just above the IC50 level to minimize the possibility of nonspecific effects. Coincubation of PD098059 or SB203580 with anti-CD3 plus anti-CD28 and 8-Br-cAMP did not result in any reversal of the cAMP-mediated inhibition of IL-5 (Table IGo). However, incubation of PBMC with PD098059 inhibited anti-CD3 plus anti-CD28-induced IL-5 release by 60%, whereas SB203580 had no effect (Table IGo).


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  		Table I. Effect of MAPK inhibitors on IL-5 production1

 
Effect of cAMP and H-89 on T cell proliferation

Using BrdU incorporation and FACS, CD3 plus CD28 costimulation resulted in a proliferative response in lymphocytes, which on account of the stimulus, must correspond to T cells (Fig. 3Go, A and B). A number of studies have shown that cAMP-elevating agents can inhibit T cell proliferation, and we have confirmed this in response to 8-Br-cAMP, forskolin, and rolipram (11, 37) (Fig. 3Go). However, the addition of H-89 (3 µM) did not prevent the antiproliferative effect of these drugs and, in fact, appeared to enhance the observed inhibition.



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  		FIGURE 3. Effect of cAMP and H-89 on T cell proliferation. PBMC were incubated with anti-CD3 plus anti-CD28 as above and coincubated with 8-Br-cAMP (1 mM), rolipram (30 µM), or forskolin (1 µM) with or without H-89 (3 µM). After 44 h, cells were incubated with BrdU (50 µM) for a further 4 h before harvesting and labeling with FITC-labeled anti-BrdU and propidium iodide (PI). A, Following FACS analysis and gating for proliferating cells, the amount of FITC-labeled anti-BrdU is plotted against propidium iodide (PI), and representative dot plots are shown. The area (R2) representing proliferating cells is shown. B, Data (i.e., cells within the R2 region as percentage of total lymphocytes) are expressed as means ± SEM of seven independent experiments. Significance was tested by Kruskal-Wallis ANOVA using Dunn’s post-test.

 
H-89 inhibits PKA activity and CREB phosphorylation

To verify that H-89 was having a functional effect on PKA activity, PBMC were coincubated with 8-Br-cAMP, rolipram, or forskolin in the presence or absence of H-89 (Fig. 4GoA). In each case, there was a significant increase in PKA activity that was abolished by H-89. Stimulation with anti-CD3 plus anti-CD28 alone had no effect on PKA activity (data not shown).



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  		FIGURE 4. H-89 inhibits PKA activity and phosphorylation of CREB. A, Cells were either not treated (nt) or incubated with 8-Br-cAMP (1 mM), rolipram (30 µM), or forskolin (1 µM) with or without H-89 (3 µM). Cells were harvested after 1 h, and PKA activity was measured. Data from seven independent experiments are expressed as means ± SEM of the fold induction of basal PKA activity. Significance was tested by Friedman ANOVA using Dunn’s post test. B, Cells were stimulated for 30 min as described above with anyi-CD3 plus anti-CD28 with combinations of 8-Br-cAMP and H-89. Total proteins were harvested for Western blot analysis. Representative blots for Ser133-phosphorylated CREB (p-CREB) and pan CREB (CREB) are shown. Data (bottom panel) are expressed as the ratio of p-CREB:CREB, and the results are expressed as means ± SEM of at least eight independent experiments. Significance was tested by Kruskal-Wallis ANOVA using Dunn’s post-test.

 
CREB is activated by PKA-dependent phosphorylation of Ser133 (19). Therefore, we used the phosphorylation status of this residue to further validate the effect of H-89. Following anti-CD3 plus anti-CD28 stimulation, no increase in CREB phosphorylation was observed (Fig. 4GoB). However, addition of 8-Br-cAMP markedly increased CREB phosphorylation, and this effect was abolished by H-89 (Fig. 4GoB).

Effect of cAMP-elevating agents on Rap1 activation

Recently, cAMP has been found to activate several GEFs that stimulate downstream GTPases and feed into MAPK signaling pathways (38). One such GEF is Epac, which can activate the small GTPase Rap1 by causing it to bind GTP. Rap1 is thought to exert at least some of its effects by binding to and activating the MKK1 kinase B-Raf (39). To investigate the possible role of the Epac/cAMP-GEF-Rap1-B-Raf pathway, Western blotting was performed for B-Raf. However, we found no evidence in PBMC lysates of the 68-kDa band that corresponds to B-Raf in positive control PC12 cells. Thus, B-Raf-dependent signaling seems unlikely. However, immunoreactive bands were observed at ~40 and 50 kDa (Fig. 5GoA). These bands were not observed in PC12 lysates, and at present, it is not clear whether these represent breakdown products of B-Raf, closely related proteins, or simply nonspecific interactions.



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  		FIGURE 5. Rap1 and B-Raf are not activated by cAMP. B, Anti-CD3 plus anti-CD28 plus 8-Br-cAMP-treated PBMC lysates and untreated PC12 lysates were analyzed by SDS-PAGE, and Western blotting for B-Raf was performed. A representative blot is shown. B, Cells were stimulated with anti-CD3 plus anti-CD28 or with 8-Br-cAMP (1 mM) as described above for 30 min. Using GST-RalGDS-RBD, activated Rap1 was affinity purified from 100 µg of each cell lysate and analyzed by Western blotting. A representative blot is shown, and data from eight independent experiments are shown as means ± SEM.

 
To study the activation status of Rap1, the GTP-bound form of Rap1 was affinity purified and analyzed by Western analysis (26). This method exploits the ability of the active GTP-bound form of Rap1 to bind the Ras binding domain (RBD) of the Ral guanine nucleotide stimulator protein (RalGDS). The RalGDS-RBD is expressed as a GST fusion protein and purified from bacterial culture, which then allows the active Rap1 to be affinity purified (26, 27). However, Rap1 activation in PBMC stimulated by anti-CD3 plus anti-CD28 appeared to be reduced. This was further reduced by 8-Br-cAMP, and the addition of H-89 seemed to reverse this effect. Although these data failed to reach statistical significance, it is clear that these results do not support a role for Rap1 in the inhibition of IL-5 by cAMP-elevating agents.


   Discussion
Top
 Abstract
 Introduction
 Materials and Methods
 Results
 Discussion
References
 
cAMP was identified as a second messenger in the 1950s and was subsequently shown to exert many of its downstream effects via activation of PKA (40). However, this paradigm has now become so entrenched that many cAMP-driven effects are simply assumed to be PKA dependent.

Gs-coupled receptors such as {beta}2-adrenoceptors or the EP2 and EP4 prostanoid receptors (41, 42) directly activate adenylate cyclase to produce a transient rise in intracellular cAMP (43). This results in activation of downstream cAMP-dependent effector molecules such as PKA. In this study, we have used separate Gs-coupled receptor-mediated stimuli, direct activation of Gs, direct activation of adenylate cyclase, and inhibition of PDE4, a cAMP-specific PDE, as well as the cAMP analog 8-Br-cAMP to inhibit IL-5 release from CD3 plus CD28-stimulated PBMC. Taken together, the use of these mechanistically distinct means of elevating cAMP strongly supports a cAMP-dependent mechanism for the observed inhibition of IL-5. However, contrary to the dogma that has been accepted in regard to smooth muscle tone (28, 29), combined treatment with forskolin and rolipram failed to elicit any additional effect over a simple additive response (Fig. 1GoC). These data suggest that the response to each compound is mechanistically distinct and, as such, requires careful examination. One explanation for this effect is that these responses are actually cAMP independent. However, we view this possibility as unlikely, given the nature of the various compounds, which include an active cAMP analog. A second, more likely, possibility is that these responses are indeed cAMP-dependent, but that there exists multiple cAMP-dependent effector mechanisms that are either spatially or temporally separated (44). Spatial separation or compartmentalization of cAMP pools is not a new hypothesis and has been invoked to explain numerous effects including the lack of a direct relationship between cAMP content and PKA activity in canine trachealis (45), the failure of rolipram to potentiate isoproterenol-induced relaxation of bronchial smooth muscle (46), and a lack of synergy between albuterol and rolipram in the repression of LPS-induced TNF-{alpha} from monocytes (47). Furthermore, in recent years, the specific activation and localization/colocalization of the multiple adenylate cyclases, PDE and PKA isoforms, and isoform splice variants have been clearly demonstrated (48, 49, 50). Thus, the activation and recruitment of the various components of the cAMP signaling pathway to precise intracellular sites via interaction with adapter or scaffold proteins may produce levels of specificity that were previously unsuspected and could easily account for the observations in this study.

A second explanation for the lack of synergy between forskolin and rolipram may lie in the temporal separation between the cause and effect. Elevation of cAMP within T cells occurs in the order of minutes (51), whereas IL-5 release was measured after 24 h. Thus, the relationship between cause and effect is unlikely to be direct and could involve multiple downstream effectors and possible de novo gene expression. Thus, confounding factors, including the various forms of desensitization and other negative feedback processes, may obscure any synergy. In addition, there is evidence that cAMP may act at multiple levels (transcription, posttranscription, or translation) to repress gene expression. For example, the ability of albuterol to inhibit eotaxin release from smooth muscle was lost if added later than 2 h following cell stimulation, suggesting a window of effectiveness that corresponds to early gene expression events such as transcription (52). Similarly, cAMP-elevating agents are known to repress NF-{kappa}B-dependent transcription by a variety of mechanisms (53). This contrasts with the ability of {beta}2-agonists to repress their own mRNA expression by posttranscriptional destabilization and the finding that, in adipocytes, cAMP-elevating agents down-regulated pathways that are involved in translational control (54, 55). Furthermore, one mechanism of growth inhibition by forskolin in lymphoid cells involved translational down-regulation of cyclin D3 (56). Thus, temporal separation may also be sufficient to account for our observations.

To explore the role of PKA in these responses, the effect of H-89, a selective inhibitor of PKA that acts by competitive inhibition of the ATP binding site, was assessed (30). However, no obvious effect in regard to IL-5 inhibition by 8-Br-cAMP, rolipram, forskolin, or PGE2 was observed. Because this finding was shared with other structurally and mechanistically distinct inhibitors of PKA, these data suggest that PKA may not play a major role in this process. Furthermore, inhibition by H-89 of the cAMP-dependent increase in both PKA activity and phosphorylation of the PKA substrate, Ser133 of CREB, confirms this hypothesis by showing that H-89 gained entry to the cells and was functionally active.

In addition to effects on cytokine release, another important property of cAMP-elevating agents is their ability to inhibit T cell proliferation (11, 37). In this respect, we have shown that the inhibition of T cell proliferation by various cAMP-elevating agents was again independent of PKA. This finding is in agreement with a recent study, in which evidence for a PKA-independent mechanism in the immunomodulatory effects of cAMP was reported, and suggests that non-PKA-dependent effects play a major role in the cAMP-dependent effector functions in T cells (57).

Collectively, the results of the present study indicate that other cAMP-driven, but PKA-independent, signaling mechanisms account for the suppression of IL-5 production from PBMC. One possible candidate for these effects is the PKG signaling pathway. PKG, which is expressed in T cells, can be directly activated by cAMP, and activation of this enzyme has been shown to inhibit IL-2 generation (33, 34). In addition, PKG may also be indirectly activated via the cAMP-dependent induction of inducible NO synthase (58, 59, 60). This enzyme produces NO, which activates soluble guanylate cyclase, which in turn increases intracellular cGMP levels and activates PKG (61). However, as the active cGMP analog, Sp-8-Br-PET-cGMPS, and the selective PKG inhibitor, Rp-8-pCPT-cGMPS, both of which have biological activity in T cells (34), had no effect on IL-5 release or on cAMP-mediated inhibition of IL-5 release, respectively, our data suggest that this effect may not be PKG mediated.

Various MAPK pathways have been implicated as downstream effectors of cAMP (62). However, use of the MKK1 inhibitor, PD098059, and p38 MAPK inhibitor, SB203580, indicated that these particular pathways are not involved in the cAMP-mediated inhibition of IL-5. This is consistent with the downstream kinase, extracellular-regulated protein kinase (ERK), being involved in TCR-stimulated release of IL-5 (63, 64). Furthermore, and in agreement with previous studies (65), we have found that 8-Br-cAMP failed to inhibit the anti-CD3 plus anti-CD28-induced rise in ERK phosphorylation (data not shown). These observations, coupled with the fact that PD098059 inhibited IL-5 release by ~60%, support a role for MKK1 in the CD3 plus CD28-dependent release of IL-5 rather than in inhibition of IL-5 release.

Other putative targets of cAMP are the cAMP-activated GEFs Epac1 and Epac2 (22, 66). In PC12 cells, these GEFs activate Rap1 to signal through the Raf pathway (21, 66). Previous studies have suggested that B-Raf, which can activate ERK, is the predominant downstream effector of Rap1 (38). However, because we failed to detect B-Raf in PBMC, together with the involvement of MKK-ERK activation in the release of IL-5, the above scheme is unlikely in T cells (63, 64). Furthermore, because 8-Br-cAMP appeared to inhibit activation of Rap1, and this effect was reversed by H-89 (Fig. 5GoB), we tentatively suggest that Rap1 activity may be negatively regulated by a PKA-dependent mechanism. These data are in contrast to the pathway described in platelets, in which a similar assay was used to show cAMP activation of Rap1 (67). Certainly, we did not observe any activation of Rap1 and can therefore exclude a role for B-Raf and Rap1 in cAMP-mediated inhibition of IL-5 release. However, this observation does not rule out roles for the Epacs/cAMP-GEFs, which may act via different downstream effectors in these cells (66).

In summary, this study excludes a role for PKA and PKG in the cAMP-dependent inhibition of IL-5 release and proliferation of T cells in a mixed PBMC population. In addition, evidence is also presented that the downstream effectors of Epac/cAMP-GEF, Rap1, and B-Raf are unlikely to be involved in the signaling downstream of cAMP in this system. Collectively, these data are highly important because, in addition to excluding a role for the above pathways, and in particular PKA, the data suggest that there is at least one uncharacterized cAMP-dependent pathway that mediates key cAMP-dependent responses in human T lymphocytes.


   Footnotes
 
1 This work was supported by a grant from Boehringer Ingelheim. M.B. is the holder of a Deutsche Forschungsgemeinschaft scholarship. Back

2 Current address: Franz-Volhard Clinic at Max-Delbrück Center, Charité, Humboldt University, Berlin, Germany. Back

3 Address correspondence and reprint requests to Dr. Robert Newton at the current address: Molecular Physiology Group, Department of Biological Sciences, University of Warwick, Gibbet Hill Road, Coventry, CV4 7AL, U.K. E-mail address: robert.newton{at}ic.ac.uk Back

4 Abbreviations used in this paper: PDE, phosphodiesterase; PK, protein kinase; GEF, guanine nucleotide exchange factor; Epac, exchange protein directly activated by cAMP; 8-Br-cAMP, 8-bromoadenosine cAMP; CTX, cholera toxin; PKI, PKA inhibitor peptide; Rp-8-CPT-cAMP, 8-(4-chlorophenylthio) adenosine-3',5'-cyclic monophosphorothioate Rp isomer; Sp-8-Br-PET-cGMPS, {beta}-phenyl-1,N2-etheno-8-bromoguanosine-3',5'-cyclic monophosphorothioate Sp isomer; Rp-8-pCPT-cGMPS, 8-(4-chlorophenylthio)guanosine-3',5'-cyclic monophosphorothioate Rp isomer; BrdU, 5-bromo-2'-deoxyuridine; MAPK, mitogen-activated protein kinase; MKK1, MAPK kinase 1; RBD, Ras binding domain; RalGDS, Ral guanine nucleotide stimulator protein; ERK, extracellular-regulated protein kinase. Back

Received for publication September 13, 2000. Accepted for publication June 12, 2001.


   References
Top
 Abstract
 Introduction
 Materials and Methods
 Results
 Discussion
 References
 

  1. Djukanovic, R., W. R. Roche, J. W. Wilson, C. R. Beasley, O. P. Twentyman, R. H. Howarth, S. T. Holgate. 1990. Mucosal inflammation in asthma. Am. Rev. Respir Dis. 142:434.[Medline]
  2. Humbert, M., C. J. Corrigan, P. Kimmitt, S. J. Till, A. B. Kay, S. R. Durham. 1997. Relationship between IL-4 and IL-5 mRNA expression and disease severity in atopic asthma. Am. J. Respir. Crit. Care Med. 156:704.[Abstract/Free Full Text]
  3. Clutterbuck, E. J., E. M. Hirst, C. J. Sanderson. 1989. Human interleukin-5 (IL-5) regulates the production of eosinophils in human bone marrow cultures: comparison and interaction with IL-1, IL-3, IL-6, and GMCSF. Blood 73:1504.[Abstract/Free Full Text]
  4. Clutterbuck, E. J., C. J. Sanderson. 1990. Regulation of human eosinophil precursor production by cytokines: a comparison of recombinant human interleukin-1 (rhIL-1), rhIL-3, rhIL-5, rhIL-6, and rh granulocyte-macrophage colony-stimulating factor. Blood 75:1774.[Abstract/Free Full Text]
  5. Giembycz, M. A., M. A. Lindsay. 1999. Pharmacology of the eosinophil. Pharmacol. Rev. 51:213.[Abstract/Free Full Text]
  6. Shichijo, M., N. Inagaki, M. Kimata, I. Serizawa, H. Saito, H. Nagai. 1999. Role of cyclic 3',5'-adenosine monophosphate in the regulation of chemical mediator release and cytokine production from cultured human mast cells. J. Allergy Clin. Immunol. 103:S421.[Medline]
  7. Salvi, S., A. Semper, A. Blomberg, J. Holloway, Z. Jaffar, A. Papi, L. Teran, R. Polosa, F. Kelly, T. Sandstrom, S. Holgate, A. Frew. 1999. Interleukin-5 production by human airway epithelial cells. Am. J. Respir. Cell Mol. Biol. 20:984.[Abstract/Free Full Text]
  8. Hamid, Q., M. Azzawi, S. Ying, R. Moqbel, A. J. Wardlaw, C. J. Corrigan, B. Bradley, S. R. Durham, J. V. Collins, P. K. Jeffery. 1991. Expression of mRNA for interleukin-5 in mucosal bronchial biopsies from asthma. J. Clin. Invest. 87:1541.
  9. Ying, S., S. R. Durham, C. J. Corrigan, Q. Hamid, A. B. Kay. 1995. Phenotype of cells expressing mRNA for TH2-type (interleukin 4 and interleukin 5) and TH1-type (interleukin 2 and interferon {gamma}) cytokines in bronchoalveolar lavage and bronchial biopsies from atopic asthmatic and normal control subjects. Am. J. Respir. Cell Mol. Biol. 12:477.[Abstract]
  10. Barnes, P. J.. 1999. Effect of {beta}-agonists on inflammatory cells. J. Allergy Clin. Immunol. 104:S10.[Medline]
  11. Bartik, M. M., G. P. Bauman, W. H. Brooks, T. L. Roszman. 1994. Costimulatory signals modulate the antiproliferative effects of agents that elevate cAMP in T cells. Cell. Immunol. 158:116.[Medline]
  12. Averill, L. E., R. L. Stein, G. M. Kammer. 1988. Control of human T-lymphocyte interleukin-2 production by a cAMP-dependent pathway. Cell. Immunol. 115:88.[Medline]
  13. Anastassiou, E. D., F. Paliogianni, J. P. Balow, H. Yamada, D. T. Boumpas. 1992. Prostaglandin E2 and other cyclic AMP-elevating agents modulate IL-2 and IL-2R{alpha} gene expression at multiple levels. J. Immunol. 148:2845.[Abstract]
  14. Giembycz, M. A.. 2000. Phosphodiesterase 4 inhibitors and the treatment of asthma: where are we now and where do we go from here?. Drugs 59:193.[Medline]
  15. Torphy, T. J.. 1998. Phosphodiesterase isozymes: molecular targets for novel antiasthma agents. Am. J. Respir. Crit. Care Med. 157:351.[Free Full Text]
  16. Conti, M. A., R. S. Adelstein. 1981. The relationship between calmodulin binding and phosphorylation of smooth muscle myosin kinase by the catalytic subunit of 3':5' cAMP-dependent protein kinase. J. Biol. Chem. 256:3178.[Abstract/Free Full Text]
  17. Samizo, K., T. Okagaki, K. Kohama. 1999. Inhibitory effect of phosphorylated myosin light chain kinase on the ATP-dependent actin-myosin interaction. Biochem. Biophys. Res. Commun. 261:95.[Medline]
  18. Roesler, W. J., G. R. Vandenbark, R. W. Hanson. 1988. Cyclic AMP and the induction of eukaryotic gene transcription. J. Biol. Chem. 263:9063.[Free Full Text]
  19. Lalli, E., P. Sassone-Corsi. 1994. Signal transduction and gene regulation: the nuclear response to cAMP. J. Biol. Chem. 269:17359.[Free Full Text]
  20. Parry, R. V., D. Olive, J. Westwick, D. M. Sansom, S. G. Ward. 1997. Evidence that a kinase distinct from protein kinase C and phosphatidylinositol 3-kinase mediates ligation-dependent serine/threonine phosphorylation of the T-lymphocyte co-stimulatory molecule CD28. Biochem. J. 326:249.
  21. de Rooij, J., F. J. Zwartkruis, M. H. Verheijen, R. H. Cool, S. M. Nijman, A. Wittinghofer, J. L. Bos. 1998. Epac is a Rap1 guanine-nucleotide-exchange factor directly activated by cyclic AMP. Nature 396:474.[Medline]
  22. Kawasaki, H., G. M. Springett, N. Mochizuki, S. Toki, M. Nakaya, M. Matsuda, D. E. Housman, A. M. Graybiel. 1998. A family of cAMP-binding proteins that directly activate Rap1. Science 282:2275.[Abstract/Free Full Text]
  23. Staples, K. J., M. Bergmann, P. J. Barnes, R. Newton. 2000. Stimulus-specific inhibition of IL-5 by cAMP-elevating agents and IL-10 reveals differential mechanisms of action. Biochem. Biophys. Res. Commun. 273:811.[Medline]
  24. Lu, X., D. P. Lane. 1993. Differential induction of transcriptionally active p53 following UV or ionizing radiation: defects in chromosome instability syndromes?. Cell 75:765.[Medline]
  25. Giembycz, M. A., J. Diamond. 1990. Partial characterization of cyclic AMP-dependent protein kinases in guinea pig lung employing the synthetic heptapeptide substrate, kemptide: in vitro sensitivity of the soluble enzyme to isoprenaline, forskolin, methacholine and leukotriene D4. Biochem. Pharmacol. 39:1297.[Medline]
  26. Franke, B., J. W. Akkerman, J. L. Bos. 1997. Rapid Ca2+-mediated activation of Rap1 in human platelets. EMBO J. 16:252.[Medline]
  27. McPhee, I., M. D. Houslay, S. J. Yarwood. 2000. Use of an activation-specific probe to show that Rap1A and Rap1B display different sensitivities to activation by forskolin in rat1 cells. FEBS Lett. 477:213.[Medline]
  28. Giembycz, M. A., D. Raeburn. 1991. Putative substrates for cyclic nucleotide-dependent protein kinases and the control of airway smooth muscle tone. J. Auton. Pharmacol. 11:365.[Medline]
  29. Torphy, T. J.. 1994. {beta}-adrenoceptors, cAMP and airway smooth muscle relaxation: challenges to the dogma. Trends Pharmacol. Sci. 15:370.[Medline]
  30. Engh, R. A., A. Girod, V. Kinzel, R. Huber, D. Bossemeyer. 1996. Crystal structures of catalytic subunit of cAMP-dependent protein kinase in complex with isoquinolinesulfonyl protein kinase inhibitors H7, H8, and H89: structural implications for selectivity. J. Biol. Chem. 271:26157.[Abstract/Free Full Text]
  31. Gjertsen, B. T., G. Mellgren, A. Otten, E. Maronde, H. G. Genieser, B. Jastorff, O. K. Vintermyr, G. S. McKnight, S. O. Doskeland. 1995. Novel (Rp)-cAMPS analogs as tools for inhibition of cAMP-kinase in cell culture: basal cAMP-kinase activity modulates interleukin-1{beta} action. J. Biol. Chem. 270:20599.[Abstract/Free Full Text]
  32. Glass, D. B., L. J. Lundquist, B. M. Katz, D. A. Walsh. 1989. Protein kinase inhibitor-(6–22)-amide peptide analogs with standard and nonstandard amino acid substitutions for phenylalanine 10: inhibition of cAMP-dependent protein kinase. J. Biol. Chem. 264:14579.[Abstract/Free Full Text]
  33. Francis, S. H., J. D. Corbin. 1999. Cyclic nucleotide-dependent protein kinases: intracellular receptors for cAMP and cGMP action. Crit. Rev. Clin. Lab. Sci. 36:275.[Medline]
  34. Fischer, T. A., A. Palmetshofer, S. Gambaryan, E. Butt, C. Jassoy, U. Walter, S. Sopper, S. M. Lohmann. 2001. Activation of cGMP-dependent protein kinase I{beta} inhibits IL-2 release and proliferation of T cell receptor-stimulated human peripheral T cells. J. Biol. Chem. 276:5967.[Abstract/Free Full Text]
  35. Alessi, D. R., A. Cuenda, P. Cohen, D. T. Dudley, A. R. Saltiel. 1995. PD 098059 is a specific inhibitor of the activation of mitogen-activated protein kinase kinase in vitro and in vivo. J. Biol. Chem. 270:27489.[Abstract/Free Full Text]
  36. Cuenda, A., J. Rouse, Y. N. Doza, R. Meier, P. Cohen, T. F. Gallagher, P. R. Young, J. C. Lee. 1995. SB 203580 is a specific inhibitor of a MAP kinase homologue which is stimulated by cellular stresses and interleukin-1. FEBS Lett. 364:229.[Medline]
  37. Giembycz, M. A., C. J. Corrigan, J. Seybold, R. Newton, P. J. Barnes. 1996. Identification of cyclic AMP phosphodiesterases 3, 4 and 7 in human CD4+ and CD8+ T-lymphocytes: role in regulating proliferation and the biosynthesis of interleukin-2. Br. J. Pharmacol. 118:1945.[Medline]
  38. Bos, J. L.. 1998. All in the family: new insights and questions regarding interconnectivity of Ras, Rap1 and Ral. EMBO J. 17:6776.[Medline]
  39. Ohtsuka, T., K. Shimizu, B. Yamamori, S. Kuroda, Y. Takai. 1996. Activation of brain B-Raf protein kinase by Rap1B small GTP-binding protein. J. Biol. Chem. 271:1258.[Abstract/Free Full Text]
  40. Kammer, G. M.. 1988. The adenylate cyclase-cAMP-protein kinase A pathway and regulation of the immune response. Immunol. Today 9:222.[Medline]
  41. Bylund, D. B., D. C. Eikenberg, J. P. Hieble, S. Z. Langer, R. J. Lefkowitz, K. P. Minneman, P. B. Molinoff, R. R. J. Ruffolo, U. Trendelenburg. 1994. International union of pharmacology nomenclature of adrenoceptors. Pharmacol. Rev. 46:121.[Medline]
  42. Coleman, R. A., W. L. Smith, S. Narumiya. 1994. International union of pharmacology classification of prostanoid receptors: properties, distribution, and structure of the receptors and their subtypes. Pharmacol. Rev. 46:205.[Medline]
  43. Gilman, A. G.. 1984. G proteins and dual control of adenylate cyclase. Cell 36:577.[Medline]
  44. Houslay, M. D., G. Milligan. 1997. Tailoring cAMP-signalling responses through isoform multiplicity. Trends Biochem. Sci. 22:217.[Medline]
  45. Zhou, H. L., S. J. Newsholme, T. J. Torphy. 1992. Agonist-related differences in the relationship between cAMP content and protein kinase activity in canine trachealis. J. Pharmacol. Exp. Ther. 261:1260.[Abstract/Free Full Text]
  46. Torphy, T. J., B. J. Undem, L. B. Cieslinski, M. A. Luttmann, M. L. Reeves, D. W. Hay. 1993. Identification, characterization and functional role of phosphodiesterase isozymes in human airway smooth muscle. J. Pharmacol. Exp. Ther. 265:1213.[Abstract/Free Full Text]
  47. Seldon, P. M., P. J. Barnes, K. Meja, M. A. Giembycz. 1995. Suppression of lipopolysaccharide-induced tumor necrosis factor-{alpha} generation from human peripheral blood monocytes by inhibitors of phosphodiesterase 4: interaction with stimulants of adenylyl cyclase. Mol. Pharmacol. 48:747.[Abstract]
  48. Hurley, J. H.. 1999. Structure, mechanism, and regulation of mammalian adenylyl cyclase. J. Biol. Chem. 274:7599.[Free Full Text]
  49. Houslay, M. D., W. Kolch. 2000. Cell-type specific integration of cross-talk between extracellular signal-regulated kinase and cAMP signaling. Mol. Pharmacol. 58:659.[Free Full Text]
  50. Feliciello, A., M. E. Gottesman, E. V. Avvedimento. 2001. The biological functions of A-kinase anchor proteins. J. Mol. Biol. 308:99.[Medline]
  51. Bartik, M. M., W. H. Brooks, T. L. Roszman. 1993. Modulation of T cell proliferation by stimulation of the {beta}-adrenergic receptor: lack of correlation between inhibition of T cell proliferation and cAMP accumulation. Cell. Immunol. 148:408.[Medline]
  52. Pang, L., A. J. Knox. 2001. Regulation of TNF-{alpha}-induced eotaxin release from cultured human airway smooth muscle cells by {beta}2-agonists and corticosteroids. FASEB J. 15:261.[Abstract/Free Full Text]
  53. Ye, R. D.. 2000. {beta}-Adrenergic agonists regulate NF-{kappa}B activation through multiple mechanisms. Am. J. Physiol. Lung Cell. Mol. Physiol. 279:L615.[Free Full Text]
  54. Danner, S., M. Frank, M. J. Lohse. 1998. Agonist regulation of human {beta}2-adrenergic receptor mRNA stability occurs via a specific AU-rich element. J. Biol. Chem. 273:3223.[Abstract/Free Full Text]
  55. Lin, T. A., J. C. J. Lawrence. 1996. Control of the translational regulators PHAS-I and PHAS-II by insulin and cAMP in 3T3-L1 adipocytes. J. Biol. Chem. 271:30199.[Abstract/Free Full Text]
  56. Naderi, S., K. B. Gutzkow, J. Christoffersen, E. B. Smeland, H. K. Blomhoff. 2000. cAMP-mediated growth inhibition of lymphoid cells in G1: rapid down-regulation of cyclin D3 at the level of translation. Eur. J. Immunol. 30:1757.[Medline]
  57. Bryce, P. J., M. J. Dascombe, I. V. Hutchinson. 1999. Immunomodulatory effects of pharmacological elevation of cyclic AMP in T lymphocytes proceed via a protein kinase A independent mechanism. Immunopharmacology 41:139.[Medline]
  58. Koide, M., Y. Kawahara, I. Nakayama, T. Tsuda, M. Yokoyama. 1993. Cyclic AMP-elevating agents induce an inducible type of nitric oxide synthase in cultured vascular smooth muscle cells: synergism with the induction elicited by inflammatory cytokines. J. Biol. Chem. 268:24959.[Abstract/Free Full Text]
  59. Benbernou, N., S. Esnault, H. C. Shin, H. Fekkar, M. Guenounou. 1997. Differential regulation of IFN-{gamma}, IL-10 and inducible nitric oxide synthase in human T cells by cyclic AMP-dependent signal transduction pathway. Immunology 91:361.[Medline]
  60. Bauer, H., T. Jung, D. Tsikas, D. O. Stichtenoth, J. C. Frolich, C. Neumann. 1997. Nitric oxide inhibits the secretion of T-helper 1- and T-helper 2-associated cytokines in activated human T cells. Immunology 90:205.[Medline]
  61. Ignarro, L. J.. 1991. Signal transduction mechanisms involving nitric oxide. Biochem. Pharmacol. 41:485.[Medline]
  62. Vossler, M. R., H. Yao, R. D. York, M. G. Pan, C. S. Rim, P. J. Stork. 1997. cAMP activates MAP kinase and Elk-1 through a B-Raf- and Rap1-dependent pathway. Cell 89:73.[Medline]
  63. Egerton, M., D. R. Fitzpatrick, A. Kelso. 1998. Activation of the extracellular signal-regulated kinase pathway is differentially required for TCR-stimulated production of six cytokines in primary T lymphocytes. Int. Immunol. 10:223.[Abstract/Free Full Text]
  64. Cantrell, D.. 1996. T cell antigen receptor signal transduction pathways. Annu. Rev Immunol. 14:259.[Medline]
  65. Hsueh, Y. P., M. Z. Lai. 1995. c-Jun N-terminal kinase but not mitogen-activated protein kinase is sensitive to cAMP inhibition in T lymphocytes. J. Biol. Chem. 270:18094.[Abstract/Free Full Text]
  66. de Rooij, J., H. Rehmann, M. van Triest, R. H. Cool, A. Wittinghofer, J. L. Bos. 2000. Mechanism of regulation of the Epac family of cAMP-dependent RapGEFs. J. Biol. Chem. 275:20829.[Abstract/Free Full Text]
  67. Altschuler, D., E. G. Lapetina. 1993. Mutational analysis of the cAMP-dependent protein kinase-mediated phosphorylation site of Rap1b. J. Biol. Chem. 268:7527.[Abstract/Free Full Text]



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