3-hydroxy-3-methylglutaryl–coenzyme A (HMG-CoA) reductase is a critical enzyme in the mevalonate pathway that regulates the biosynthesis of cholesterol as well as isoprenoids that mediate the membrane association of certain GTPases. Blockade of this enzyme by atorvastatin (AT) inhibits the destructive proinflammatory T helper cell (Th)1 response during experimental autoimmune encephalomyelitis and may be beneficial in the treatment of multiple sclerosis and other Th1-mediated autoimmune diseases. Here we present evidence linking specific isoprenoid intermediates of the mevalonate pathway to signaling pathways that regulate T cell autoimmunity. We demonstrate that the isoprenoid geranylgeranyl-pyrophosphate (GGPP) mediates proliferation, whereas both GGPP and its precursor, farnesyl-PP, regulate the Th1 differentiation of myelin-reactive T cells. Depletion of these isoprenoid intermediates in vivo via oral AT administration hindered these T cell responses by decreasing geranylgeranylated RhoA and farnesylated Ras at the plasma membrane. This was associated with reduced extracellular signal–regulated kinase (ERK) and p38 phosphorylation and DNA binding of their cotarget c-fos in response to T cell receptor activation. Inhibition of ERK and p38 mimicked the effects of AT and induced a Th2 cytokine shift. Thus, by connecting isoprenoid availability to regulation of Th1/Th2 fate, we have elucidated a mechanism by which AT may suppress Th1-mediated central nervous system autoimmune disease.
Recently, it was reported that oral administration of simvastatin (Zocor) reduced the expected number of new gadolinium-enhancing lesions in relapsing-remitting multiple sclerosis (MS) patients by 44% in a small 6-mo open-label trial (1). The related drug atorvastatin (AT) (Lipitor) has also shown promising results in lowering disease scores and vascular risk factors in patients with rheumatoid arthritis (2) and is currently being tested in MS in a multicenter, placebo-controlled trial (http://www.immunetolerance.org/trials) (3). Studies in experimental autoimmune encephalomyelitis (EAE) (4–8) and other animal models of Th1-mediated disease (9, 10) have revealed that statin drugs interfere with the autoimmune destruction of target tissues by inhibiting multiple arms of the immune response.
In EAE, statins prevent the production of inflammatory mediators TNF-α, IFN-γ, and iNOS by astrocytes and microglia in the central nervous system (CNS) (4) and blunt inducible expression of MHCII and costimulatory molecules by these cells (5). These drugs also affect T cells, the initiators of the autoimmune process, by preventing their expansion, Th1 differentiation, and migration across the blood–brain barrier (5–8). When myelin-reactive CD4+ T cells are primed with antigen in the presence of statins, they instead secrete lower amounts of TNF-α and the Th1 cytokine IFN-γ and higher amounts of protective Th2 cytokines such as IL-4 (5, 6, 8). Adoptive transfer studies have demonstrated that AT-generated, myelin-reactive Th2 cells have a limited capacity to migrate into the CNS (unpublished data) and provide sustained protection from further attacks of paralysis (5). Interestingly, a similar bias toward a higher ratio of Th2/Th1 CD4+ cells in peripheral blood has been observed in human cardiac patients receiving low-dose (20 mg/d) AT therapy (11).
Despite these advances, the molecular mechanism by which statins modulate T cell immunity is unknown. This is important given the broad clinical administration of these agents (∼25 million people world-wide) (12). Identified protein targets of these drugs include 3-hydroxy-3-methylglutaryl–coenzyme A (HMG-CoA) reductase, a rate- limiting enzyme in the mevalonate pathway that generates cholesterol and isoprenoid derivatives (Fig.1 A
) (13, 14) and the integrin, leukocyte function antigen-1 (15). In the present study, we provide novel evidence that the Th2 bias promoted by AT is the result of a reduction of the mevalonate pathway-derived isoprenoids, farnesyl-pyrophosphate (PP) and all-trans geranylgeranyl-PP in T cells. These lipid derivatives are known to covalently attach to and mediate the membrane association of certain signaling proteins and metabolites in cells (13, 14). We show that in vivo depletion of these lipids in EAE mice via oral AT administration prevented the membrane association of farnesylated Ras and geranylgeranylated RhoA, but not other GTPases in lymph node cells. This was associated with compromised TCR-induced activation of Ras and RhoA effectors such as extracellular signal–regulated kinase (ERK), p38, and their cotarget c-fos. Because c-fos (as part of AP-1) transactivates the IFN-γ promoter and represses the IL-4 promoter (16), our results explain how AT can bias naive CD4+ T cells to produce relatively higher amounts of IL-4 in the early period of antigen signaling and thus trigger the Th2 program of differentiation. By connecting specific isoprenoids in the mevalonate pathway to T cell receptor signaling pathways that regulate cytokine production, we have elucidated a mechanism of how statins may inhibit Th1-mediated autoimmunity.
AT prevents Th1 differentiation of CD4+ cells by targeting HMG-CoA reductase
Previous reports have shown that the effect of AT in T cells is reversed by mevalonate (5, 6), suggesting that the actions of this drug may be mediated through inhibition of HMG-CoA reductase (Fig. 1 A). However, because statins are structurally similar to mevalonate and have other ligands on immune cells (i.e., leukocyte function antigen-1) (15), it is also possible that such a reversal is a result of competition between mevalonate and AT for binding on protein targets other than HMG-CoA reductase. We thus tested whether the effects of AT on T cells could also be reversed by farnesyl-PP, the last common intermediate in the mevalonate pathway that has a different structure than mevalonate. In response to αCD3/αCD28 costimulation, purified naive (CD62L+/CD44low) CD4+ T cells proliferated and differentiated to secrete high amounts of the Th1 cytokine IFN-γ (Fig. 1 B). As shown previously (5, 6, 8), AT blunted these T cell responses and enhanced their production of IL-4 (Fig. 1 B). Farnesyl-PP, like mevalonate, fully reversed the effects of AT and, when administered alone, enhanced the TCR-induced proliferation of CD4+ cells (Fig. 1 B).
Paralleling these in vitro findings, administration of farnesol, a lipophilic, alcohol precursor to farnesyl-PP (17), reversed the clinical and immune modulatory effects of AT in vivo during EAE (Fig. 1, C and D, and Table S1). Interestingly, myelin (PLP p139-151)-reactive cells taken from mice treated with farnesol alone also proliferated more vigorously and secreted higher amounts of IFN-γ ex vivo in response to stimulation with specific peptide (Fig. 1 D). Collectively, these findings confirm that AT modulates the Th differentiation of CD4+ cells by inhibiting the production of an intermediate in the mevalonate pathway. They also suggest that accumulation of farnesyl-PP in response to farnesol treatment may enhance the expansion of Th1 effector cells.
Effects of AT on T cell growth and differentiation are independent of cholesterol reduction
Cholesterol is a major product of farnesyl-PP (Fig. 1 A). Although it has been reported that depletion of this lipid in T cells can attenuate TCR signaling by disruption of cholesterol-rich lipid rafts (18), a recent in vitro study of malignant T cells showed lipid raft disruption by statins only in the complete absence of exogenous cholesterol in the media (19). We found that in the context of the whole organism, AT treatment (10 mg/kg) reduced the production of this metabolite by the liver as indicated by an elevation in the mRNA expression of HMG-CoA reductase (this gene is negatively regulated by sterols in this tissue; reference 13) (Fig. 2 A
). However, the total amount of cholesterol in the serum or in T cells was unchanged by this treatment (Fig. 2, B and C). The level of membrane-associated cholesterol was also not altered in T cells in response to oral administration of this drug as assessed via flow cytometric analysis of filipin staining (Fig. 2 D, left). The lack of detectable change in membrane cholesterol with AT was not a result of limits in the sensitivity of this assay, because decreased filipin fluorescence was observed in T cells incubated in serum-free media with the cholesterol-depleting agent β-methyl cyclodextrin (Fig. 2 D, right).
To more specifically address the role of the sterol branch of the mevalonate pathway in immunomodulation, we examined the effects of the squalene synthetase inhibitor Zaragozic Acid A (10 mg/kg) on encephalitogenic T cell responses during EAE. At this dose, Zaragozic Acid A inhibits liver sterol synthesis (20), reduces circulating cholesterol (Fig. 3 A
) and at the same time causes an accumulation of farnesol in mice (20). Daily subcutaneous injection of mice with Zaragozic Acid had opposite effects to AT and caused PLP p139-151–reactive cells to proliferate more vigorously (Fig. 3 B) and secrete higher amounts of IFN-γ (Fig. 3 C) and lower amounts of IL-4 (Fig. 3 D) compared with PBS-injected counterparts. Zaragozic Acid A treatment also exacerbated EAE at several time-points in disease (Fig. 3 E and Table S2).
To examine whether the enhanced proliferation of Th1 cells triggered by Zaragozic Acid A was a result of enhanced flux of farnesyl-PP into isoprenoid branches of the pathway, we investigated the effect of this drug on the de novo incorporation [1-3H] farnesyl-PP into T cell proteins in vitro. We found that in comparison to media control, Zaragozic Acid A– treated T cells displayed an increased abundance of tritium-labeled proteins in the 21–29 kD range, which is compatible with the size of small G proteins (Fig. 3 F). Collectively, these results suggest that the major effects of AT on Th1 differentiation and clinical disease are cholesterol independent and instead the result of reductions in isoprenoid biosynthesis.
AT inhibits T cell growth and Th1 differentiation by preventing protein isoprenylation
Farnesyl-PP serves as a metabolic precursor to a variety of isoprenoid derivatives such as decaprenyl-PP (isoprenoid moiety of ubiquinone), 2-cis-geranylgeranyl-PP (important for N-glycoprotein synthesis), and all-trans geranylgeranyl-PP (13, 14) (Fig. 1 A). The latter isoprenoid along with farnesyl-PP are, respectively, attached to the COOH terminus of certain signaling proteins via the action of geranylgeranyl transferases and farnesyltransferase (21). These isoprenoid modifications mediate the membrane association of many GTPases (21). We thus tested whether specific isoprenoid derivatives could reverse the effects of AT on T cells cultured with specific peptide. Splenocytes from MBP Ac1-11 TCR transgenic (Tg) mice were used as a source of T cells for these assays.
Of all the metabolites tested, only all-trans geranylgeranyl-PP, the isoprenoid moiety of geranylgeranylated proteins, and its precursor, farnesyl-PP, restored the antigen-driven proliferation of AT-treated T cells and reversed the Th2 bias promoted by this drug (Fig.4 A
). The doses of farnesyl-PP and geranylgeranyl-PP used in these assays were effective at restoring the prenylation of protein targets (Fig. 4 C). We also tested the effects of these isoprenoids in AT-treated T cells stimulated with α-CD3 and α-CD28 (Fig. S1) and found that both farnesyl-PP and geranylgeranyl-PP contributed to the reversal of AT effects on T cell proliferation and Th1 differentiation. Collectively, these data strongly suggest that AT modulates Th differentiation by inhibiting isoprenoid production in T cells.
To confirm the involvement of isoprenylated proteins in T cell growth and Th1 differentiation, we investigated the effects of inhibitors of farnesyltransferase (FTI-277) and geranylgeranyltransferase-I (GGTI-298) on antigen-driven T cell responses (Fig. 4, B and D). Treatment of MBP Ac1-11 TCR Tg T cells with an effective dose (Fig. 4 D) of the geranylgeranyltransferase inhibitor (GGTI) significantly inhibited T cell proliferation (Fig. 4 B). However, the growth of these cells was not altered by treatment with the farnesyltransferase inhibitor (FTI) (Fig. 4 B). Consistent with the prominent involvement of protein farnesylation in regulating Th1 differentiation, FTI-277 inhibited the production of IFN-γ and induced a subtle increase in IL-4 by T cells (Fig. 4 B). In parallel, this drug decreased T-bet protein and caused a subtle increase in GATA-3 expression (Fig. 4 E). GGTI-298, though not influencing IFN-γ secretion or T-bet expression, induced low-level IL-4 production and a subtle increase in GATA-3 expression (Fig. 4, B and E). Similar effects of FTI-277 and GGTI-298-treatment on T proliferation and cytokine production were observed in cultures of purified T cells stimulated with anti-CD3 and anti-CD28 (Fig. S1). Note that in both of these T cell assays, the amount of IL-4 triggered by each of these prenyltransferase inhibitors did not approach the level induced by AT (Fig. 4 B and Fig. S1), suggesting that geranylgeranylated proteins cooperate with farnesylated proteins to fully repress the production of this Th2 cytokine in T cells in response to antigen signals. Collectively, these results suggest that AT prevents T cell proliferation and Th1 differentiation by inhibiting the biosynthesis of farnesyl-PP and all-trans geranylgeranyl-PP, leading to reduced prenylation of protein targets.
Oral AT administration promotes a Th2 bias by decreasing the membrane association of Ras and RhoA
Farnesylated Ras and geranylgeranylated Rac1, RhoA, and Rap are the only prenylated proteins known to be situated in antigen-activated signaling pathways that modulate T helper differentiation (22). Though numerous in vitro studies of malignant cells have demonstrated an inhibitory effect of high-dose (10–50 μM) statin treatment on the prenylation and membrane-association of Ras and Rho GTPases (e.g., 19, 23, 24), a similar in vivo effect of statins on these proteins has not been reported. We thus investigated whether oral AT administration altered the subcellular localization of Ras, RhoA, Rac1, or Rap in T cells in vivo during EAE. We used draining lymph nodes from EAE mice as a source of enriched T cells. We found that AT treatment induced an accumulation of Ras, Rap, and RhoA, but not Rac1 in the cytosol of draining lymph node cells (Fig. 5 A
). This was accompanied by a prominent decrease in Ras and RhoA at the membrane (Fig. 5 A). This effect of AT on Ras and Rho was reversed by coadministering farnesol to mice (Fig. S2 A). Time-course experiments demonstrated that the alteration in Ras and RhoA localization in immune cells by AT was transient (Fig. 5 B) and occurred as early as 6 h (not depicted) and as late as 20 h (Fig. 5 B) after oral treatment. Because membrane localization is requisite to the functioning of these proteins, our findings strongly implicate Ras and RhoA as the major targets of AT in immune modulation.
It has been suggested that early cytokine production by naive CD4+ cells in response to antigen stimulation may be influenced by the extent of activation of the Ras–ERK signaling pathway downstream of the TCR (16, 25). In response to strong TCR signals, Ras and ERK are activated in a sustained fashion leading to increased c-fos activity (16, 25). c-fos (together with jun proteins such as AP-1) transactivates the IFN-γ promoter and may repress the IL-4 promoter (16) (Fig. 6 A
). Decreased RhoA activation may also tip cytokine balance toward Th2 via inhibition of p38, a kinase that positively regulates IFN-γ production (26) (Fig. 6 A). We thus tested whether AT treatment compromised the TCR-induced activation of ERK and p38 kinases in lymph nodes during EAE. Consistent with effects on Ras and RhoA, in vivo AT treatment blunted the TCR-induced activation of ERK and p38 as well as decreased the DNA-binding of c-fos (a target of ERK and p38) and ATF-2 (a target of p38 and JNK) (Fig. 6, C and D). This effect of AT treatment on T cell ERK and p38 phosphorylation was reversed by cotreatment of mice with farnesol (Fig. S2 B). Consistent with the lack of a major effect of AT on the subcellular localization of Rac1, this drug did not modulate JNK phosphorylation nor the activity of its primary target, c-jun (Fig. 6, C and D). Oral AT treatment also did not inhibit other signaling events triggered by anti-CD3 or anti-CD28 cross-linking including IκB degradation (Fig. 6 C), Zap-70 phosphorylation (Fig. 6 E), and calcium flux (Fig. 6 F).
To test the hypothesis that this inhibition of Ras-ERK and RhoA-p38 signaling by AT was responsible for the Th2 bias induced by this drug, we explored the effects of specific inhibitors of MEK (PD98059), an upstream effector of ERK, and p38 (SB203580) on the antigen-driven differentiation of naive CD4+ cells. Exposure of CD4+ cells to 10 μM of the MEK inhibitor (a dose that does not affect the proliferation or viability of T cells; unpublished data) decreased the production of IFN-γ and increased the secretion of IL-4 by these cells in response to specific peptide (Fig. 7 A
). This concentration of PD98059 also reduced the phosphorylation of ERK (Fig. 7 A, bottom). Similarly, exposure of T cells to the p38 kinase inhibitor at doses that inhibit p38 phosphorylation (Fig. 7 B, bottom) and activity (26) induced IL-4 production (only at 0.1 μM) and inhibited IFN-γ production by these cells (Fig. 7 B). The p38 kinase inhibitor also had a more profound effect than the MEK inhibitor in inhibiting T cell proliferation through higher doses tested (10–100 μM) (unpublished data). Collectively, these data support the hypothesis that Ras-ERK and RhoA-p38 signaling pathways are the targets of AT in Th2 differentiation and inhibition of T cell growth.
In vivo treatment with an FTI prevents Th1 differentiation during EAE
In light of the more prominent involvement of protein farnesylation and ERK signaling in regulating the Th1 differentiation of MBP-reactive cells in vitro and reports that FTIs (but not GGTIs) are well tolerated in mice (27), we investigated the clinical benefits of the FTI, L-744,832 (30 mg/kg) on the development of EAE (Fig. 8, A–D
). We administered the maximum tolerated dose of this drug, which is reported to cause regression of Ras-related tumors in mice (28). Similar to in vitro findings using FTI-277 (Fig. 4 B), IFN-γ production by PLP p139-151–reactive cells from L-744,832–treated mice was markedly reduced compared with control counterparts (Fig. 8 C). Despite this, FTI-treated mice still developed EAE, albeit the day of onset of clinical symptoms for grade one or higher (12.7 ± 0.6 in FTI vs. 11.3 ± 0.6 in vehicle, P < 0.01) and or grade two or higher (19.4 ± 2.0 in FTI vs. 16.0 ± 1.8 in vehicle, P < 0.01) was significantly delayed compared with vehicle controls (Fig. 8 A). The development of inflammation in FTI-treated mice may relate to the fact that this drug caused PLP p139-151–reactive cells to secrete higher amounts of IL-2 (Fig. 8 B), yet did not promote IL-4 secretion (not depicted) nor dampen the production of the proinflammatory cytokine TNF-α by these cells (Fig. 8 D). Collectively, these results suggest that dual inhibition of protein farnesylation and geranylgeranylation is required to fully promote a Th2 bias of CD4+ cells and prevent the development of CNS inflammation during EAE.
Several studies have demonstrated that in vivo statin treatment can cause a protective Th2 bias in animal models of Th1-mediated autoimmune disease (for review see reference 3). These findings have created considerable enthusiasm for testing these agents in patients with MS and rheumatoid arthritis (1, 2). The purpose of the present study was to define the mechanism of immune modulation by this drug. Here, we show that the effect of AT in causing a Th2 bias is the result of a reduction in the biosynthesis of isoprenoids that serve as membrane attachments for Ras and RhoA. Farnesyl-PP, which mediates Ras farnesylation, restored IFN-γ production by AT-treated myelin-reactive T cells, whereas all-trans- geranylgeranyl-PP, the precursor to RhoA geranylgeranylation, reversed the AT block in T cell proliferation and coordinated with farnesyl-PP to fully reverse the increase in IL-4 promoted by this drug. We also show for the first-time that oral dosing with AT compromised the membrane association of Ras and RhoA GTPases and the TCR-induced activation of targets ERK and p38 in T cells. Inactivation of ERK and p38 signaling mimicked the effects of AT, strongly implicating Ras-ERK and RhoA-p38 pathways as the targets of this drug. Thus, by linking isoprenoid intermediates to two arms of the TCR signaling cascade that modulate T cell cytokine production, we have elucidated a mechanism of how statins may cause a Th2 bias in vivo during EAE.
Our finding that oral dosing with AT caused Ras, RhoA, and Rap GTPases to be preferentially diverted to the cytosol instead of the membrane of lymph node cells in vivo is the first demonstration of its kind. These results thus expand upon previous in vitro reports of lovastatin in tumor cell lines (19, 23, 24) as well as lend concrete support to the prevailing notion that the pleiotrophic effects of statins in treating atherosclerosis and cancer in animal models are the result of reductions in isoprenoid biosynthesis (29–32). Though oral AT administration significantly depleted Ras and RhoA at the membrane of lymph node cells, in comparison, Rap or Rac1 were only marginally affected. The reason for this difference is unclear, but may relate to variations in the half-lives of these proteins (24). Nonetheless, because membrane-association is necessary for the functioning of GTPases, we conclude that Ras and RhoA are the major targets of statin in immune modulation in vivo.
Previous reports have demonstrated that the strength of ERK activation in response to TCR stimulation may influence cytokine production and alter the course of T helper differentiation by altering the binding of c-fos to AP-1 consensus elements (16). Peptides that bind the TCR with strong avidity induce Th1 differentiation of CD4+ cells and cause a sustained activation of Ras and ERK that triggers c-fos activity (16, 25). c-fos (with jun as AP-1) appears to repress the IL-4 promoter (16) and coordinates with other transcription factors such as ATF-2 and NFAT to mediate the transactivation of the IFN-γ promoter (26) (Fig. 6 A). However, under conditions when ERK activity is low, such as in the presence of a weak-binding altered peptide ligand (16), or weakened Ras (33), or MEK signaling (16, 34), IFN-γ production is minimal and IL-4 is induced. In this regard, our findings that AT decreased the DNA binding of c-fos and inhibited the activation or Ras-ERK and RhoA-p38 signaling pathways that target this transcription factor provide a mechanistic explanation for the Th2 bias promoted by statins. Interference of p38 activity by AT may have also contributed to this Th2 deviation by reducing the activity of ATF-2 at the IFN-γ promoter (26). In light of this evidence, we propose a model for AT action on T cells in vivo (Fig. 6, compare A and B), whereby this drug selectively inhibits the membrane association of Ras and RhoA leading to decreased activation of ERK and p38 signaling pathways that target AP-1 and ATF-2.
Despite the established role for Ras and ERK in the regulation of IFN-γ production (in this paper and references 16, 33, 34), in vivo FTI treatment only delayed the onset of EAE. These findings emphasize the involvement of geranylgeranylated proteins in mediating the development of CNS inflammation. Indeed, our data indicate a role for geranylgeranylated Rho proteins in mediating the proliferation of encephalitogenic T cells. These results thus correspond with previous reports that statins cause G1 arrest (35) and that geranylgeranylated proteins regulate the G1 to S transition (36). We also found that inhibition of protein geranylgeranylation in myelin-reactive cells was requisite for full induction of IL-4 and was likely required for the attenuation of TNF-α production by AT (i.e., AT [reference 5], but not FTI treatment diminishes T cell production of this cytokine). These findings, coupled with the established involvement of geranylgeranylated Rho proteins in regulating the transmigration of T cells across brain endothelium (7), emphasize that dual inhibition of farnesylation and geranylgeranylation by statins is necessary to prevent the development of CNS autoimmunity.
Although reducing the production of farnesyl-PP by AT hindered T cell growth and Th1 differentiation, in vivo treatments that cause increased incorporation of this metabolite into prenylated proteins, such as farnesol (17) or Zaragozic Acid A (18, 37), induced pathogenic myelin-reactive T cells to proliferate more vigorously, secrete higher amounts of IFN-γ, and precipitate worse EAE. Thus, accumulation of farnesyl-PP may enhance Th1-mediated inflammation in vivo. Though we observed in vitro Zaragozic Acid A treatment to trigger an increased accumulation of farnesyl-PP in T cells, it remains unclear whether this also occurred in mice in response to in vivo treatment or whether it was the increased liver production of farnesyl-PP–derived lipids (18, 37) that was responsible for the immune modulatory effects of this drug. The latter possibility (i.e., that the liver production of isoprenoids can boost adaptive immune responses) is provocative and provides an interesting correlate to reports that metabolic precursors in the mevalonate pathway are preferentially diverted toward isoprenoid as opposed to sterol biosynthesis in the liver during the acute phase response to inflammatory stimuli (38, 39).
In conclusion, we show that farnesylated Ras and geranylgeranylated RhoA proteins are the targets of AT in immune modulation in vivo. Our results also underscore that inhibition of both protein farnesylation and geranylgeranylation in T cells is key to promoting a Th2 bias and preventing the development of EAE. Because oral AT administration is well tolerated, whereas continuous and combined FTI and GGTI therapy is toxic in vivo (27), we maintain that of these, statin treatment is a more promising approach than selective inhibition of individual prenyltransferases for treatment of MS and other Th1-mediated autoimmune diseases.
Materials And Methods
Mevalonate, farnesol, farnesyl-PP, all-trans geranylgeranyl-PP, ubiquinone, Zaragozic Acid A, β-methyl cyclodextrin, and filipin were obtained from Sigma-Aldrich. Cold 2-cis geranylgeraniol, [acetyl-3H] acetyl CoA (20 Ci/mmol), and [1-3H] farnesyl-PP (60 Ci/mmol) were obtained from American Radiochemicals. Purified AT was a gift from R. Laskey (Pfizer, New York, NY). FTI-277, GGTI-298, L-744,832, SB203580, and PD98059 were obtained from Calbiochem. Fluo-4 was obtained from Invitrogen. Peptides encoding myelin basic protein (MBP), Ac1–11 (Ac-ASQKRPSQRHG), or proteolipid protein (PLP) p139–151 (HCLGKWLGHPDKF) were synthesized by the Stanford Pan Facility and purified by HPLC. Pan Ras (clone 18) and Rac1 (clone 102) antibodies were obtained from BD Transduction Labs. RhoA (clone 26C4), Rap1 (clone sc-65), T-bet (clone sc-21749), and GATA-3 (clone sc-268) antibodies were obtained from Santa Cruz Biotechnology, Inc. Phospho(p42/44)-ERK (no. 9101S), p42/p44 MAPK (no. 9102), phospho-JNK (no. 9251S), JNK (no. 9252), phospho-p38 (no. 9216S), p38 (no. 9212), phospho-Zap-70 (no. 2701), and IκBα (no. 9242) antibodies were all obtained from Cell Signaling. The pan-Zap-70 antibody (clone 1E7.2) was obtained from Upstate Biotechnology. Goat anti–mouse IgG antibody was obtained from Jackson ImmunoResearch Laboratories.
Female SJL/J and (PL/J × SJ/L)F1 mice (6–10 wk old) were purchased from The Jackson Laboratory. MBP Ac1-11 TCR Tg mice backcrossed onto the B10.PL background (40) were maintained in our animal facility. All animal protocols were approved by the Division of Comparative Medicine at Stanford University and the Committee of Animal Research at the University of California San Francisco and animals were maintained in accordance with the guidelines of the National Institutes of Health.
EAE was induced in SJL/J mice via subcutaneous immunization with 100 μg PLP p139-151 in an emulsion (volume ratio 1:1) with CFA containing 4 mg/ml of heat-killed Mycobacterium tuberculosis H37Ra (Difco Laboratories). (PL/J × SJ/L)F1 mice were immunized with MBP Ac1-11 in CFA. Mice (n = 10 per treatment group) were examined daily for clinical signs of EAE and were scored as followed: 0 = no clinical disease, 1 = limp tail, 2 = hindlimb weakness, 3 = complete hindlimb paralysis, 4 = hindlimb paralysis plus some forelimb paralysis, and 5 = moribund or dead.
In vivo drug treatments.
AT (prescription formulation; Pfizer) was brought into suspension in PBS (0.4 mg/ml) and a 0.5-ml volume of this suspension (equivalent to 10 mg/kg) was administered to mice orally, once daily, using 20-mm feeding needles (Popper and Sons, Inc). Farnesol (undiluted lipid, 5 mg/kg) and Zaragozic Acid A (dissolved in saline, 10 mg/kg) were injected i.p. once daily. The specific inhibitor of farnesyltransferase, L-744,832, was dissolved in 0.9% saline (pH 5.4, 30 mg/kg) and injected subcutaneously, once daily. Mice treated with appropriate vehicles served as controls. All treatments were initiated at 2 d before immunization, and splenocyte and lymph node cells were harvested from representative mice in each group at 10 d after disease induction.
Proliferation assays and cytokine analysis.
Splenocytes (0.5 × 106 cells/well), lymph node cells (0.5 × 106 cells/well), or CD4+ T cells (5 × 104 cells/well) purified by negative selection (columns from R&D Systems) were cultured in flat-bottomed, 96-well plates with appropriate peptide (1–25 μg/ml) and irradiated splenocytes (in the case of purified CD4+ cells) or were stimulated with 2 or 5 μg/ml each of αCD3 (clone 145-2C11; BD Biosciences) and αCD28 (clone 37.51; BD Biosciences). Culture medium consisted of RPMI 1640 supplemented with l-glutamine (2 mM), sodium pyruvate (1 mM), nonessential amino acids (0.1 mM), penicillin (100 U/ml), streptomycin (0.1 mg/ml), 2-mercaptoethanol (5 × 10−5 M), and 10% fetal calf serum. After 48–72 h, cultures were pulsed with [3H]thymidine (1 μCi/well) and 18 h later were harvested onto filter paper. The cpm of incorporated [3H]thymidine were read using a β-counter. Cytokines were measured in the supernatants of cultured cells using anti–mouse OPTEIA ELISA kits (BD Biosciences). Supernatants were taken at the time of peak production for each cytokine: IL-2 (48 h), IFN-γ (72 h), TNF-α (72 h), and IL-4 (120 h).
Analysis of HMG-CoA reductase mRNA expression via real-time RT-PCR.
Total RNA was isolated from liver using the Absolutely RNA RT-PCR Miniprep kit (Statagene). 1 μg of RNA was reverse-transcribed and HMG-CoA reductase and β actin cDNAs amplified according to previous methods (41) using a Lightcycler (Roche). Primer sequences were as follows: HMG-CoA reductase (sense): 5′-TTCTGGCAGTCAGTGGG-3′; HMG-CoA reductase (antisense): 5-CAATGTTTGCTGCGTGG-3′; β-actin (sense): 5′-GAACCCTAAGGCCAACGCT-3′; and β-actin (antisense): 5′-CACGCACGATTTCCCTCTC-3′.
T cell cholesterol extraction and amplex red assay.
Total cholesterol was extracted from cells using the Heider and Boyett method (42). In brief, purified cells (10 × 106) were suspended in 500 μl of isopropanol and sonicated for 15 s using a microprobe. Samples were centrifuged at 800 g for 15 min to precipitate cellular proteins. The supernatant containing the cholesterol was decanted to a clean tube, evaporated to dryness, and resuspended in 1× reaction buffer. The remaining protein pellet was suspended in 100 μl of 0.1 M sodium hydroxide and used for protein determination. Total cholesterol was measured in the lipid extract and in serum of mice using Amplex Red Cholesterol Assay kit (Invitrogen).
FACS analysis of filipin staining.
Membrane-associated cholesterol was determined in T cells by measuring filipin fluorescence (43). T cells (106) were first fixed in 120 μl of 4% paraformaldehyde at room temperature for 12 min, washed three times in 1× PBS, and incubated with the dye (1:100 of 25 mg/ml filipin stock) for 1 h at 4°C. Samples were washed three times with 1× PBS and filipin fluorescence was measured using a FACS Vantage SE/Diva (BD Biosciences) with the krypton ion laser tuned to UV (350.7–356.4 nm) and emission detection at 420–460 nm. Data were analyzed using FloJo software (Ver. 6.3.3) (Treestar).
De novo incorporation of farnesyl-PP into T cell proteins was assessed using a modified procedure of Corsini et al. (44). In brief, purified T cells (3 × 106/ml in stimulation media) were cultured in six-well plates coated with anti-CD3 (5 μg/ml) and anti-CD28 (5 μg/ml) in the absence or presence of 200 μM Zaragozic Acid A. After 12 h, T cells were pulsed with [1-3H] farnesyl-PP (60 Ci/mmol) and cultured for additional 20 h. For each condition, cells were pooled and washed three times in 1× PBS (containing 1 mM PMSF). After the final centrifuge (1,200 revolutions/min for 5 min), cells were resuspended in 1× PBS and sonicated for 15 s using a microprobe. Cellular proteins were delipidated (44), 60 μg of protein was subjected to SDS-PAGE, and gels were stained with Coomassie blue to visualize proteins. Gels were then treated with Amplify for 30 min, washed, dried, and exposed to a Tritium K-Screen (Kodak) for 3 wk. Exposure of the screen was detected using a Fx Pro-Plus Molecular Imager and Quantity One software (both obtained from Bio-Rad Laboratories).
Cell fractionation and protein isolation.
For extraction of total cell protein, splenocytes or lymph node cells were dissociated from surrounding connective tissue, red blood cells were lysed, and cells were counted and resuspended in an appropriate volume (10 μl/million cells) of NP-40 buffer (150 mM NaCl, 1 mM EDTA, 1 mM EGTA, 1% Triton X-100, 2.5 mM Na2PO4, 1 mM glycerol phosphate, 1 mM Na3V04, 1 g/ml leupeptin, 1 mM PMSF, Roche protease inhibitor tablet, 20 mM Tris, pH 7.5). After a 30-min extraction on ice, samples were centrifuged at 15,000 g for 15 min at 4°C to obtain a clarified supernatant. For cell fractionation studies, splenocyte or lymph node cells were homogenized in lysis buffer (1 mM EDTA, 20 mM Tris-HCl, pH 7.4) using a glass homogenizer and were centrifuged at 100,000 g using a Beckman ultracentrifuge. The supernatant (soluble fraction) was concentrated using a 10 K molecular limit Nanosep centrifugal device (Pall Life Sciences). The membrane pellet was solubilized in 1× immunoprecipitation buffer (0.15 M NaCl, 1% Triton X-100, 0.5% sodium deoxycholate, and 0.1% SDS, 10 mM Tris-HCl, pH 7.5) and centrifuged at 15,000 g to obtain a clarified supernatant. Proteinase inhibitors were included in all buffers. Nuclear extracts from lymph nodes cells were isolated using the BD Transfactor Extraction Kit (CLONTECH Laboratories, Inc.) according to kit directions. The concentration of proteins in each sample was determined using a BCA assay kit (Pierce Chemical Co.). DNA binding assays were conducted using a commercial ELISA kit (CLONTECH Laboratories, Inc.).
SDS-PAGE and Western analysis.
Each protein sample was suspended in 2 vol. of 2× SDS Sample Buffer (Bio-Rad Laboratories) and subjected to SDS-PAGE electrophoresis using precast Tris-HCl Ready-Gels (Bio-Rad Laboratories). Proteins were transferred to PVDF membranes (GE Healthcare) and immunoblotting was performed using conventional methods (Santa Cruz Biotechnology, Inc.).
Calcium flux analysis.
Calcium flux in CD4+ T cells was measured after CD3 cross-linking using a FACScan (BD Biosciences) (45). In brief, CD4+ cells purified from spleens of mice (106/ml), were washed in 1× PBS and loaded with Fluo-4 (2 μM) in the presence of CaCl2 (2 mM) for 20 min at room temperature. Cells were washed twice with 1× PBS, resuspended at a concentration of 2 × 106/ml in FACS buffer, and placed in a 37°C water bath. Samples (37°C) were first acquired for 30 s to establish baseline fluorescence in FL1 channel before the addition of anti-CD3 (5 μg/ml) and the goat anti–mouse IgG (10 μg/ml). After stimulation, events were collected for an additional 10 min. Data were analyzed using the kinetics platform in FloJo software (Ver. 6.3.3).
Data are presented as means ± SE. When data were parametric, a one-way analysis of variance and a Scheffé post-hoc test (for >2 groups) or a Student's t test (n = 2 groups) were used to detect between-group differences. When data were nonparametric, ranks were compared amongst groups using a Kruskal-Wallis test and nonparametric test for multiple comparisons (for >2 groups) or a Mann-Whitney U test (n = 2 groups). A value of P < 0.05 was considered significant.
Online supplemental material.
Fig. S1 shows the influence of AT and isoprenoid metabolites on the proliferation of and cytokine production by purified T cells in culture. Fig. S2 shows how in vivo treatment with farnesol can reverse the effects of AT on the membrane localization of Ras and RhoA and the TCR-induced phosphorylation of ERK and p38 in lymph node cells. Tables S1 and S2 summarize the clinical features of EAE in experiments depicted in Figs. 1 and 3.
We thank Dr. R. Laskey for providing us with purified atorvastatin. We thank C. Haines for help with the calcium flux assay and E. Middleman for help with radiography. We also thank S. Ousman for insightful comments on the manuscript.
S.E.D. is supported by postdoctoral fellowships from the National Multiple Sclerosis Society (NMSS) and Canadian Multiple Sclerosis Society. S.Y. is supported by a postdoctoral fellowship from the NMSS. Support for this research was provided by the National Institutes of Health (grant no. RO1AI05709), the NMSS (grant no. RG 3622-A), and the Wadsworth Foundation (to S.S. Zamvil and L. Steinman).
The authors have no conflicting financial interests.
Abbreviations used: AT, atorvastatin; CNS, central nervous system; EAE, experimental autoimmune encephalomyelitis; ERK, extracellular signal–regulated kinase; FTI, farensyltransferase inhibitor; GGTI, geranylgeranyltransferase inhibitor; HMG-CoA, 3-hydroxy-3-methylglutaryl–coenzyme A; MS, multiple sclerosis; PP, pyrophosphate; Tg, transgenic.
S.E. Dunn and S. Youssef contributed equally to this work.
S.S. Zamvil and L. Steinman contributed equally to this work.