Impaired degranulation but enhanced cytokine production after FcRI stimulation of diacylglycerol kinase –deficient mast cells
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《实验药学杂志》
1 The Signal Transduction Program, The Abramson Family Cancer Research Institute and 2 The Department of Medicine, University of Pennsylvania School of Medicine, Philadelphia, PA 19104
3 Department of Pediatrics and 4 Department of Immunology, Duke University Medical Center, Durham, NC 27710
CORRESPONDENCE Gary Koretzky: koretzky@mail.med.upenn.edu OR Xiao-Ping Zhong: zhong001@mc.duke.edu
Calcium and diacylglycerol are critical second messengers that together effect mast cell degranulation after allergen cross-linking of immunoglobulin (Ig)E-bound FcRI. Diacylglycerol kinase (DGK) is a negative regulator of diacylglycerol-dependent signaling that acts by converting diacylglycerol to phosphatidic acid. We reported previously that DGK–/– mice have enhanced in vivo T cell function. Here, we demonstrate that these mice have diminished in vivo mast cell function, as revealed by impaired local anaphylactic responses. Concordantly, DGK–/– bone marrow–derived mast cells (BMMCs) demonstrate impaired degranulation after FcRI cross-linking, associated with diminished phospholipase C activity, calcium flux, and protein kinase C–?II membrane recruitment. In contrast, Ras-Erk signals and interleukin-6 production are enhanced, both during IgE sensitization and after antigen cross-linking of FcRI. Our data demonstrate dissociation between cytokine production and degranulation in mast cells and reveal the importance of DGK activity during IgE sensitization for proper attenuation of FcRI signals.
Abbreviations used: BMMC, bone marrow–derived cell; DAG, diacylglycerol; DGK, DAG kinase; IP3, inositol 1,4,5-trisphosphate; LAT, linker for activated T cells; MAPK, mitogen-activated protein kinase; PA, phosphatidic acid; PCA, passive cutaneous anaphylaxis; PI5K, phosphatidylinositol 4-phosphate 5-kinase; PIP2, phosphatidylinositol 4,5-bisphosphate; PKC, protein kinase C; PLC, phospholipase C.
B.A. Olenchock and R. Guo contributed equally to this work.
Mast cells play important roles in both innate and adaptive immune responses. They are central effector cells in immune responses to parasites and in the pathogenesis of diseases such as asthma and allergy (1, 2). The high affinity receptor for IgE (FcRI) is one of several cell surface receptors critical for mast cell development and function (3). FcRI binds to IgE in the absence of antigen and subsequent cross-linking of IgE-bound FcRI by cognate antigen induces a signaling cascade that leads to mast cell degranulation and cytokine secretion, which contribute to both chronic allergic inflammation and acute anaphylaxis. Understanding FcRI signaling and mast cell activation is critical to devising new therapies for mast cell–mediated diseases.
Recent studies have greatly improved our understanding of FcRI signaling. After FcRI engagement, the Src family members Lyn and Fyn and the tyrosine kinase Syk are activated (4, 5). These molecules in turn recruit and activate other kinases such as the Tec family kinase Btk (6), phospholipid modifying enzymes including phosphatidylinositol 4,5-bisphosphate 3-kinase (PI3K) (7), the GTPase-activating molecule Vav1 (8), and adaptor molecules such as linker for activated T cells (LAT) (9), non– T cell activation linker (NTAL/LAB) (10, 11), SH2 domain containing leukocyte phosphoprotein of 76 kD (SLP-76) (12, 13), and Grb2-associated binder protein 2 (Gab2) (14). The formation of a multimolecular signaling complex coordinates activation of various downstream signaling pathways necessary for mast cell effector functions. These pathways include phospholipase C (PLC) (15, 16), protein kinase C (PKC) isoforms (17, 18), and mitogen-activated protein kinases (MAPKs) (19). PLC hydrolyzes the membrane phospholipid phosphatidylinositol 4,5-bisphosphate (PIP2), leading to the generation of two important second messengers, diacylglycerol (DAG) and inositol 1,4,5-trisphosphate (IP3). IP3 binds to its receptor in the endoplasmic reticulum and induces Ca2+ release into the cytoplasm. DAG recruits to the membrane and activates PKC family members and RasGRPs, which are recently identified guanine nucleotide exchange factors for Ras and Rap (20). Synergistic action of multiple downstream signals, particularly Ca2+ and PKCs, are required to induce mast cell degranulation (18, 21, 22). Activated PKCs and MAPKs together promote transcription of many proinflammatory genes, including cytokines (22–25).
Both in vitro and in vivo evidence suggest a critical role for DAG in the regulation of mast cell function after FcRI engagement. Treatment of mast cells with DAG analogues in the presence of a Ca2+ ionophore can mimic FcRI engagement and induce mast cells to degranulate and release active mediators (26, 27). Mice lacking PLC2, the enzyme that generates IP3 and DAG, have diminished mast cell function (28, 29). Similarly, deficiency in DAG effector molecules alters mast cell function. Multiple PKCs are expressed in mast cells, and activation of both classical and novel isoforms of PKC is regulated by DAG (18, 30). Different PKCs have distinct functions in mast cells. PKC?–/– mast cells demonstrate decreased IL-6 production and degranulation in response to FcRI engagement (22), whereas PKC–/– mast cells respond more vigorously to suboptimal FcRI stimulation with more sustained Ca2+ mobilization and increased degranulation compared with WT mast cells (31). Thus, proper balance of PKC? and PKC activities appears important for mast cell function.
These observations suggest that DAG levels must be tightly controlled in mast cells. One mechanism for terminating DAG signaling is by phosphorylation catalyzed by the DAG kinase (DGK) family of enzymes. Phosphorylation of DAG by DGKs converts DAG to phosphatidic acid (PA), thus preventing DAG from activating PKCs and RasGRPs (20, 32–34). Additionally, PA itself is a second messenger, and DGK activity could regulate mast cell function by affecting PA accumulation. In vitro, PA is a potent activator of PLC and phosphatidylinositol 4-phosphate 5-kinase (PI5K), enzymes involved in PIP2 degradation and production (35–37). Therefore, through conversion of DAG into PA, DGK enzymes could regulate many aspects of inositol lipid metabolism and mast cell activation after FcRI engagement.
We recently described mice deficient in DGK and demonstrated that T cells from these animals are hyper-responsive to TCR stimulation. DGK–/– mice mount enhanced antiviral immune responses, indicating that DGK is an important in vivo negative regulator of TCR signaling and T cell activation (38, 39). We show here that DGK also regulates immune receptor signaling in mast cells. To our surprise, in vivo mast cell function is impaired in DGK–/– mice as indicated by diminished local anaphylactic responses. To explore the mechanism underlying this finding, we have studied DGK–/– bone marrow–derived mast cells (BMMCs). We demonstrate that FcRI-induced degranulation of DGK–/– BMMCs is diminished, correlating with impaired PLC activation and PKC?II membrane translocation. Similar to what we have observed after TCR stimulation, however, FcRI-induced activation of the Ras–Erk signaling pathway is enhanced and DGK–/– BMMCs produce increased IL-6 during IgE sensitization and after antigen cross-linking of the FcRI. Moreover, mast cell survival after growth factor withdrawal is greatly increased by DGK deficiency, correlating with maintained phosphorylation of Akt. These findings indicate that DGK functions to maintain mast cell responsiveness to antigen stimulation during passive sensitization with IgE and demonstrate separation of cytokine production and degranulation after FcRI stimulation of mast cells.
RESULTS
Mast cells develop in DGK-deficient mice
We previously reported that DGK plays an important role in T cell activation (38, 39). DGK is also expressed in mast cells and, as in T cells, the 115-kD isoform is prominent (Fig. 1 A ). There are also smaller species reactive with the anti-DGK antibody, which may be products of protein degradation, as mast cells are rich in granules containing proteases. Alternatively, these might represent products of alternate transcripts. Importantly, the three major species reactive with the DGK antibody are all absent in BMMCs from targeted mice (Fig. 1 A). Mast cell development is unaffected by DGK deficiency for the following reasons: the numbers of mast cells in ear, skin, stomach, and spleen are similar in WT and DGK–/– mice (Fig. 1 B and not depicted); electron microscopy did not reveal any differences in cell morphology or number of intracellular granules (not depicted); and KO mast cells express similar levels of c-Kit and FcRI on their surfaces (Fig. 1 C). Additionally, DGK deficiency does not result in compensatory up-regulation of transcripts for related DGK isoforms (Fig. S1, available at http://www.jem.org/cgi/content/full/jem.20052424/DC1).
Figure 1. DGK expression and surface expression of FcRI and c-Kit in BMMCs from WT and DGK-deficient mice. (A) DGK protein in cell lysates made from WT and DGK-deficient BMMCs was detected by Western blot analysis using an antibody specific for the carboxyl-terminus of DGK (reference 71). The arrow indicates the 115-kD 1 isoform. (B) Mast cell distribution in the skin. Mast cells in the skin (back) and ears were stained with toluidine blue and were counted under a light microscope. Data shown are the means ± standard error of the number of mast cells per high-power field (10 x 100). (C) FcRI and c-Kit expression on BMMCs. For FcRI expression, WT and DGK-deficient BMMCs were incubated with 1 μg/ml anti-DNP IgE for 4 h (solid line) and FcRI expression was detected by staining with a FITC-labeled anti-IgE secondary antibody. Cells that had not been incubated with IgE serve as a control (dotted line). For c-Kit expression, WT and DGK-deficient BMMCs were either stained with a PE-labeled control antibody (dotted line) or a PE-labeled anti–c-Kit antibody (solid line).
Decreased passive cutaneous anaphylaxis in DGK-deficient mice
DGK–/– T cells have enhanced homeostatic proliferation and antiviral responses in vivo (39). To test the importance of DGK in mast cell function, we assessed allergic responses by examining passive cutaneous anaphylaxis (PCA), an in vivo measure of FcRI-dependent mast cell function. Unexpectedly, DGK–/– mice had significantly impaired localized anaphylactic responses (Fig. 2 A ).
Figure 2. Decreased passive cutaneous anaphylaxis and FcRI-induced degranulation but increased IL-6 production as the result of DGK deficiency. (A) WT and DGK–/– mice were injected subcutaneously with 25 ng IgE in 25 μl PBS in the right ear and with 25 μl PBS in the left ear. 24 h later, DNP-HSA and Evans blue dye were injected intravenously into the mice. 30 min after injection, tissue from the ears was collected, Evans blue was extracted, and the intensity of the dye was measured by absorption at 610 nm (OD610). Each data point is OD610 of IgE-injected ear minus the OD610 of PBS-injected ear from the same mouse. Data shown comprise three experiments. (B) Decreased FcRI-induced degranulation in DGK–/– BMMCs. IgE-sensitized WT and DGK–/– BMMCs were left unstimulated or were stimulated with various concentrations of DNP-HSA at 37°C for 60 min. Cells were spun, and ?-hexosaminidase activities in supernatants as well as in whole cell lysates of unstimulated BMMCs were measured. Data were calculated as percentage of ?-hexosaminidase activity in the supernatant to the activity in the whole cell lysates of the same genotype. Means ± standard error of triplicates are shown. Data are representative of three experiments. (C) Increased IL-6 production in DGK-deficient BMMCs. WT and DGK-deficient BMMCs were left unstimulated, were stimulated with 1 μg/ml IgE overnight, or were sensitized with 1 μg/ml IgE for 4 h and cross-linked with 30 ng/ml DNP-HSA overnight. IL-6 in the culture medium was measure by ELISA. Data shown are means ± standard error of triplicates normalized to PMA/Io control and are representative of three experiments.
To explore why DGK–/– mice demonstrate impaired PCA responses, we first compared FcRI-triggered degranulation in WT versus DGK–/– BMMCs by measuring ?-hexosaminidase release (Fig. 2 B). FcRI-induced degranulation was significantly diminished in DGK–/– BMMCs (Fig. 2 B). PMA plus ionomycin (Io) stimulation, however, resulted in similar degranulation in WT and DGK–/– BMMCs, indicating that the ability to release granules and total granule content is unaffected by DGK deficiency. The impairment of FcRI-induced mast cell degranulation likely contributes to the decreased PCA responses in DGK–/– mice.
Another consequence of FcRI engagement is the production of proinflammatory cytokines such as IL-6. IgE alone can induce a significant amount of IL-6 production in WT BMMCs (Fig. 2 C), which is consistent with previous reports (40). Cross-linking the receptor with antigen induces even more IL-6 production. Under both stimulation conditions, DGK–/– BMMCs produce approximately twofold more IL-6 than WT BMMCs. Therefore, DGK deficiency impairs FcRI-induced degranulation, but increases cytokine production after IgE sensitization and after cross-linking of the receptor with antigen.
Antigen stimulation of IgE-sensitized BMMCs
Cross-linking of IgE-bound FcRI results in activation of a signaling network that coordinates mast cell effector functions. To investigate why DGK–/– BMMCs have impaired degranulation but enhanced cytokine production after FcRI stimulation, we assessed how DGK deficiency affects antigen-induced FcRI signaling in IgE-sensitized BMMCs. We first verified that DGK phosphorylates DAG after antigen stimulation of BMMCs by measuring PA production. Addition of DNP-HSA to IgE-sensitized WT BMMCs results in robust PA accumulation beginning 5–10 min after stimulation (Fig. 3 A ). As expected, antigen stimulation of DGK–/– BMMCs results in significantly less PA accumulation.
Figure 3. Antigen stimulation of IgE-sensitized BMMCs. (A) DGK deficiency impairs PA production by BMMCs after FcRI stimulation. BMMCs were sensitized for 4 h with IgE, labeled with 32P-orthorphosphate, and either left unstimulated or stimulated with 10 ng/ml DNP-HSA for 10 min. Lipids were extracted, separated by TLC, and quantified using a phosphorimager. PA, the product of DAG phosphorylation, was identified by comigration with a standard. Data are presented as fold-induction calculated by cpm of stimulated cells divided by cpm of unstimulated cells. Means ± standard error of four experiments are shown; *, P < 0.05. (B–D) WT and DGK–/– BMMCs were sensitized with IgE for 4 h and left unstimulated (U) or were stimulated either with 4 ng/ml of DNP-HSA for different times or with 100 ng/ml PMA (P) for 5 min. (B) AKT phosphorylation was assessed by immunoblot analysis using an antibody specific for phosphorylated Ser473 of Akt. Total Akt is shown as a loading control. (C) Active Ras in lysates was measured by affinity precipitation using GST-Raf-RBD agarose beads followed by immunoblot analysis. (D) MEK1/2 and ERK1/2 activity was assessed by immunoblot analysis using phospho-specific antibodies. Total MEK1/2 and ERK1/2 serve as loading controls. (E) Membrane recruitment of PKC?II is diminished in DGK–/– BMMCs. IgE-sensitized BMMCs were left unstimulated (–) or were stimulated with 50 ng/ml DNP-HSA (DNP) or PMA (P) for 10 min. Triton-soluble membrane fractions were prepared and membrane translocation of PKC isoforms was determined by Western blot using antibodies to PKC?II, PKC, and calnexin (CNX) as a loading control. One representative blot is shown and data from five (PKC?II) or three (PKC) experiments were quantified and normalized to CNX; combined data are represented graphically.
We next examined signaling pathways that have been implicated in cytokine production after FcRI ligation. Activation of the PI3K/Akt and Ras/Erk pathways is required for cytokine production (23, 25, 41). Low dose stimulation of IgE-sensitized WT BMMCs with DNP-HSA weakly activates Akt, but stimulation of DGK–/– BMMCs results in significantly increased Akt activation (Fig. 3 B). FcRI activation of Ras is believed to be the result of Grb2-SOS activation (42, 43), but recent reports suggest that DAG might contribute to Ras activation through allosteric activation of the Ras guanine-nucleotide exchange factor RasGRP4 (44–46). As shown in Fig. 3 C, FcRI-induced Ras activity is enhanced in DGK–/– BMMCs. Consistent with the increased Ras activation, we observed enhanced and prolonged Mek1/2 and Erk1/2 phosphorylation in DGK–/– BMMCs compared with WT BMMCs (Fig. 3 D). The effect of DGK deficiency is selective, however, as FcRI-induced activation of the MAPKs p38 and Jnk is similar in WT and DGK–/– BMMCs (unpublished data). These data demonstrate that DGK deficiency enhances FcRI-induced activation of Akt, Ras, and Erk1/2, likely contributing to enhanced cytokine production.
Activation of PKC family members by DAG and Ca2+ coordinates mast cell degranulation after FcRI stimulation (22, 47). As expected, antigen cross-linking induces membrane recruitment of PKC?II and PKC in WT BMMCs (Fig. 3 E). However, we find that membrane recruitment of PKC?II is clearly diminished in DGK–/– BMMCs, whereas PKC recruitment is preserved. Unstimulated IgE-sensitized DGK–/– BMMCs also demonstrate diminished levels of membrane-associated PKC?II but normal PKC levels. Moreover, treatment with the DAG analogue PMA, which is not a DGK substrate and should be unaffected by DGK deficiency, results in impaired movement of PKC?II to the membrane in DGK–/– BMMCs but normal movement of PKC (Fig. 3 E, representative blot and graphical summary of replicates). The block in PKC?II recruitment was not the result of diminished protein levels, however, as total levels of PKC?II and PKC in whole cell lysates were not decreased in DGK–/– BMMCs as compared with WT BMMCs (Fig. S2, available at http://www.jem.org/cgi/content/full/jem.20052424/DC1). These data provide a likely mechanism for the impaired degranulation we observe in DGK–/– BMMCs, as FcRI cross-linking results in less recruitment of a positive regulator (PKC?II) of mast cell degranulation, but appropriate recruitment of a negative regulator of mast cell degranulation (PKC). The data also suggest that DGK is essential for FcRI activity in addition to its effect on DAG levels, as PMA and PMA/Io (unpublished data) fail to restore PKC?II recruitment in DGK–/– BMMCs.
Calcium response and PLC activity in DGK–/– BMMCs
The diminished membrane recruitment of the Ca2+-dependent PKC?II along with the preserved movement of the Ca2+-independent PKC led us to question whether DGK deficiency affects FcRI-induced Ca2+ flux. Compared with WT BMMCs, DGK–/– BMMCs have a significantly diminished Ca2+ response after FcRI stimulation by antigen (Fig. 4 A ). Consistent with the decreased Ca2+ response, phosphorylation of PLC1 and PLC2 after stimulation of the FcRI was decreased in DGK–/– BMMCs (Fig. 4 B). As tyrosine phosphorylation of PLC does not always correlate with its enzymatic activity (48), we analyzed PLC activity by assessing metabolism of the PLC substrate PIP2 and production of IP3. After receptor cross-linking in WT BMMCs, PIP2 levels quickly decrease (Fig. 4 C), and IP3 levels increase (Fig. 4 D) as a result of PLC activity. Upon stimulation of DGK–/– BMMCs, we do not observe a decrease but rather a slight increase in PIP2 levels (Fig. 4 C), and IP3 generation is impaired (Fig. 4 D). These data provide compelling evidence that DGK deficiency impairs activation of PLC after antigen stimulation of IgE-sensitized mast cells.
Figure 4. Decreased Ca2+ responses and PLC activity in DGK–/– mast cells. WT and DGK–/– BMMCs were sensitized for 4 h with IgE in cytokine-free media. (A) Deceased Ca2+ flux in DGK–/– mast cells after FcRI stimulation. WT and DGK–/– BMMCs were loaded with Indo-1 and stimulated with 100 ng/ml DNP-HSA to induce Ca2+ responses. Ca2+ flux was determined by flow cytometry based on the change of FL5/FL4 ratio. Data shown are representative of four experiments. (B) Decreased PLC phosphorylation in DGK–/– BMMCs after FcRI stimulation. BMMCs were stimulated with different concentrations of DNP-HSA for 2 min. PLC phosphorylation was determined by Western blot with anti–phospho- PLC1 and anti–phospho-PLC2 antibodies. The blots were probed with an anti-actin antibody as a loading control. (C) Decreased PIP2 hydrolysis in DGK–/– BMMCs. Cells were labeled with 32P-orthophosphate and stimulated for the indicated amounts of time with 10 ng/ml DNP-HSA; lipids were analyzed as in Fig. 3. PIP2 was identified by comigration with a standard. Data are means ± standard error of four different experiments. *, P = 0.01, 0.5 min stimulation, WT vs. DGK KO. (D) Diminished IP3 generation in DGK–/– BMMCs. Cells were left unstimulated or were stimulated with 10 ng/ml DNP-HSA for 20 s or 2 min and lysed using perchloric acid, and IP3 was measured.
IgE signaling and function in the absence of antigen
IgE sensitization of DGK–/– BMMCs leads to increased cytokine production and impaired PKC?II recruitment to the membrane, so we therefore examined how IgE alone signaling and function is altered in DGK deficiency. IgE binding to FcRI induces a large increase in PA in WT BMMCs (Fig. 5 A ). DGK–/– BMMCs, in contrast, have a significant impairment in PA accumulation during IgE sensitization. DAG-dependent signaling is also enhanced in DGK–/– BMMCs during IgE sensitization, as Ras and Erk1/2 activity is enhanced (Fig. 5 B).
Figure 5. IgE stimulation in the absence of antigen cross-linking results in enhanced signaling in DGK–/– BMMCs. BMMCs were rested in media without cytokines for at least 4 h and rested for 1 h in Tyrode's buffer before stimulation. (A) Impaired PA production in DGK–/– BMMCs. Cells were labeled with 32P-orthophosphate for 1 h and stimulated with 1 μg/ml IgE for 30 min. Lipids were extracted and PA production was quantified as in Fig. 3. Means ± standard error of five experiments are shown. *, P < 0.05. (B) Enhanced Ras/ERK activation in DGK–/– BMMCs. BMMCs were stimulated with 1 μg/ml IgE for various amounts of time or with 100 ng/ml PMA for 5 min. Active Ras and ERK1/2 phosphorylation were assessed as in Fig. 3. For the Ras blot, a space is included before the PMA lanes to designate that these samples were run on a separate gel.
IgE binding to the FcRI signals mast cell survival through up-regulation of antiapoptotic proteins (40, 49–52), and ex vivo mast cell survival and expansion requires IL-3 (53, 54). In the presence of IL-3, both WT and DGK–/– mast cells survive and expand similarly (unpublished data). When IL-3 is withdrawn, WT BMMCs undergo apoptosis as expected (Fig. 6 A ). Surprisingly, DGK–/– BMMCs have greatly enhanced survival in the absence of IL-3. IgE enhances survival in both WT and DGK–/– BMMCs, but because survival in the absence of cytokines is so much greater in the DGK–/– BMMCs, the IgE survival effect is less marked (Fig. 6, A and B).
Figure 6. Enhanced survival of DGK–/– BMMCs after IL-3 withdrawal. WT and DGK–/– BMMCs were cultured in media without cytokines in the presence of different concentrations of IgE for 48 or 110 h. Survival of BMMCs was determined by staining with FITC-annexin V and PI and analyzed by flow cytometry. (A) Representative dot-plots. (B) Percentage of live cells (Annexin-V and PI negative) in a full time course and at a range of concentrations of IgE. Data shown are representative of three experiments. (C) Akt phosphorylation during growth in cytokine-replete media (+IL3/SCF) and after 18 h cytokine withdrawal (18 h, no cytokines) was assessed by immunoblot analysis. One representative blot is shown and data from three independent experiments were quantified, normalized to PLC1 signal, and represented graphically for comparison. P-AKT signal in WT cells grown in cytokine-replete media was arbitrarily set to 1.
Akt regulates cell survival and is activated by IgE binding to FcRI (40). Akt is phosphorylated in WT BMMCs grown in cytokine-replete media, and this activation decreases after withdrawal of cytokines (Fig. 6 C). DGK–/– BMMCs, in contrast, have enhanced Akt activity during growth in cytokine-replete media and maintain Akt activity after cytokine removal (Fig. 6 C). As cytokines stimulate inositol metabolism, including PIP2 hydrolysis by PLC and phosphorylation by PI3K (55, 56), it is likely that DGK regulates signals generated through cytokine receptors in addition to its role in FcRI signaling. Future work will explore the biochemical basis of this observation.
DISCUSSION
We have studied mice that lack a key enzyme involved in DAG metabolism, DGK, to address the consequences of dysregulated DAG accumulation after immune receptor signaling. We demonstrated recently that DGK functions as a key negative regulator of TCR signaling and T cell activation (38, 39). We show here that DGK plays an important and unexpected role in regulating signal transduction from the FcRI in mast cells. DGK–/– BMMCs manifest decreased PA production, enhanced activation of the Ras-Mek-Erk signaling pathway, increased Akt phosphorylation, prolonged survival after cytokine deprivation, and enhanced production of IL-6 as compared with WT BMMCs. Surprisingly, IgE-mediated PCA responses are significantly decreased in DGK–/– mice, concordant with impairment of receptor-induced PLC activity and degranulation in DGK–/– BMMCs. We demonstrate that signals generated by IgE in the absence of antigen cross-linking are enhanced in DGK–/– BMMCs. These data demonstrate that DGK is important for inactivation of DAG-mediated signaling pathways in mast cells and that DGK also plays a critical role in maintaining FcRI responsiveness to antigen cross-linking. In addition, we demonstrate a novel FcRI signaling alteration in DGK–/– BMMCs, in that receptor engagement results in poor PLC activity and degranulation but augmented cytokine production.
The observation that DGK deficiency impairs PLC function after FcRI stimulation of mast cells was unexpected, as DGK was predicted to function downstream of PLC. It is possible that enhanced DAG-dependent signaling during IgE sensitization of DGK–/– BMMCs promotes feedback inhibition of PLC and Ca2+ responses upon antigen cross-linking of the FcRI. Short pretreatment of mast cells with phorbol esters results in feedback inhibition of PLC that is mediated by PKC and PKC (57–59). Prolonged administration of phorbol esters, in contrast, down-regulates PKC isoforms and potentiates PLC activity upon antigen stimulation (59). We do not see changes in PKC protein levels in DGK–/– BMMCs, and we report impaired PLC activity. PKC feedback inhibition might be indirect as well, as PKC? can induce serine-phosphorylation of Btk at an inhibitory site, dampening Btk activation in mast cells (60). Btk phosphorylates and activates PLC after FcRI stimulation, so feedback inhibition of Btk could contribute to diminished PLC activity (61). Alternatively, enhanced Erk activation in DGK–/– BMMCs could inhibit PLC association with LAT, as has been observed in T cells after TCR engagement (62). However, we have not observed an obvious decrease in PLC2-LAT association in DGK–/– BMMCs after antigen cross-linking of the FcRI (unpublished data).
Alternatively, diminished PLC activity and PKC?II membrane recruitment might be a direct consequence of DGK deficiency. Although DGK activity terminates DAG signaling, it also creates PA (32, 33, 63). PA is a potent activator of PLC enzymatic activity in vitro (35). In addition, a recent report suggests that DGK, through production of PA, may increase intracellular PIP2 by activation of PI5K I (37). Thus, DGK deficiency could lead to decreased PI5K activity, diminishing levels of the PLC substrate PIP2. Our PIP2 measurements did not reveal any differences in 32P incorporation into PIP2 in IgE-sensitized BMMCs (unpublished data), but more direct measures of PIP2 mass should be performed to ensure that steady state levels of 32P-labeled PIP2 reflect total mass. The importance of diminished PA production to the phenotype of DGK–/– BMMCs is particularly difficult to assess, as alternative pathways to generate PA exist. These pathways include the hydrolysis of phosphatidylcholine mediated by phospholipase D and the acylation of lyso-PA by lyso-PA acyltransferases (63). phospholipase D–derived PA has been reported to regulate diverse cellular processes, particularly in vesicle transportation and exocytosis (64, 65). It is possible that PA generated by DGK performs a similar function to promote mast cell degranulation.
It is intriguing that membrane recruitment of PKC?II is diminished in unstimulated IgE-sensitized DGK–/– BMMCs and that PKC?II recruitment is not restored with PMA treatment. PMA is a DAG analogue and is not subject to phosphorylation by DGK, so we predict that if DGK acts only by regulating DAG levels, PMA treatment should restore PKC?II membrane recruitment. It is possible that DGK has adaptor functions in addition to its role in lipid metabolism, perhaps by participating in a complex with PKC?II or Btk directly (37, 66). Future work will explore this interesting observation.
We have been unable to directly measure an FcRI- induced change in DAG mass in WT or DGK–/– mast cells using standard biochemical approaches (unpublished data). The likely explanation is that the receptor-induced pool of DAG is a small fraction of the total cellular pool because DAG is important for other aspects of cell biology. We are currently developing imaging approaches to measure DAG localization using a fluorescently labeled DAG probe (67). We also will develop HPLC/MS/MS techniques to quantify particular DAG subspecies, which may be more markedly regulated than total cellular DAG (68). These approaches will allow us to measure dynamic changes in DAG localization after FcRI stimulation as well as assess in vivo substrate specificity of DGK.
The increased Akt phosphorylation in DGK–/– BMMCs stimulated through cytokine or FcRs is intriguing. It is possible that increased Akt activity is a consequence of greater PIP3 production in DGK–/– BMMCs, and preliminary data support this hypothesis. Decreased PA production in DGK–/– BMMCs might increase PI3K activity, as PA has been reported to inhibit this enzyme in vitro (69). Also, perhaps decreased PLC activity in DGK–/– BMMCs increases the local concentration of PIP2 available as substrate for PI3K (66). The interrelation among different PI metabolites is complex and understanding the exact lipid alterations will require further study.
Our current studies of DGK in mast cells reveal important roles for this enzyme in regulating FcRI signaling. DGK is not only essential for terminating DAG activity but also appears to be critical for maintaining optimal FcRI responsiveness to antigen cross-linking. A more complete understanding of the importance of DGK activity to mast cell function requires analysis of other DGK family members. Ongoing biochemical and genetic studies are addressing this question.
MATERIALS AND METHODS
DGK-deficient mice.
DGK–/– mice have been described previously (39) and were housed in pathogen-free facilities at the University of Pennsylvania and Duke University. All experiments using animals were performed in accordance with regulations of the Institutional Animal Care and Use Committee of the University of Pennsylvania and Duke University.
Microscopic analysis of mast cells.
Skin samples from the back of the trunk and the ears were collected from killed WT and DGK–/– mice. Tissues were fixed and mounted in paraffin according to standard histological procedures. Paraffin sections were stained with toluidine blue and mast cells in tissues were evaluated by microscopy. In each tissue, mast cells were counted in 10 contiguous high-power fields (10 x 100).
BMMCs.
BM cells from tibias and femurs from WT and DGK–/– mice were harvested and incubated with Isocove's medium (Mediatech, Inc.) supplemented with 15% FBS (Hyclone), 100 U/ml penicillin G, 100 U/ml streptomycin, and 292 μg/ml of L-glutamine, 10 mM Hepes (pH 7.4), 0.1 mM nonessential amino acid, 1 mM sodium pyruvate, and 50 μM 2-mercaptoethanol (IMDM-15) with IL-3–conditioned medium for 2 wk and further expanded for an additional 2–8 wk with the supplement of SCF-conditioned medium made from cell lines engineered to produce these cytokines (70).
Flow cytometry.
BMMCs were analyzed directly or after 4-h sensitization with 1 μg/ml IgE. Cells were stained with fluorescently labeled antibodies in 5% FBS in PBS and were analyzed on a FACSCaliber (Becton Dickinson) with CELLQuest software. Antibodies used were PE-conjugated c-Kit and FITC-conjugated anti-IgE (BD Biosciences). To measure cell survival after cytokine withdrawal, cells were stimulated in IMDM-15 without cytokine at a concentration of 106 cells/ml in a 96-well plate with different concentrations of anti-DNP–IgE (0, 0.04, 0.2, 1, or 5 μg/ml; Sigma-Aldrich). After 48 or 110 h incubation, cells were stained with propidium iodide and annexin V–FITC (BD Biosciences) and were analyzed by flow cytometry.
Measurement of PA and PIP2.
BMMCs were sensitized at 37°C for 4 h in 1 μg/ml IgE in IMDM-15 without IL-3 or SCF. Cells were harvested and rested in Tyrode's buffer (10 mM Hepes, pH 7.4, 130 mM NaCl, 1 mM MgCl2, 5 mM KCl, 1.4 mM CaCl2, 5.6 mM glucose, and 1 mg/ml bovine serum albumin) for 1 h at 37°C. 32P-phosphoric acid (MP Biomedicals) was added to a concentration of 0.25 mCi/ml. Cells were left unstimulated or were stimulated with 10 ng/ml DNP-HSA. Stimulation was terminated by addition of 0.1 volume of ice-cold 2 M HCl and transfer of cells to ice for 10 min. Lipids were extracted with 3 ml of 2:1 methanol:chloroform and phases were separated by addition of 2 ml 1 N NaCl and 2 ml of chloroform. Lipid phase was washed 1x with 3 ml of upper phase buffer (upper phase of 10:10:9 chloroform:methanol:1 M NaCl), dried under nitrogen, and separated by thin-layer chromatography using a basic solvent (9:7:2 chloroform: methanol: 4 M NH4OH). PA and PIP2 were identified by comigration with standards (Sigma-Aldrich) and quantified using a phosphorimager.
Measurement of IP3.
IgE-sensitized BMMCs were rested for 1 h in Tyrode's buffer, then left unstimulated or stimulated for 20 s or 2 min with 10 ng/ml DNP-HSA. Stimulations were terminated by addition of 0.2 vol 20% perchloric acid for 20 min on ice. Proteins were sedimented and supernatants were neutralized to pH 7.5 by titration of 1.5 M KOH 60 mM Hepes containing universal indicator dye (Sigma-Aldrich). KClO4 was precipitated by centrifugation and IP3 was measured in supernatants by radioreceptor assay according to the manufacturer's protocol (PerkinElmer).
Western blot analysis.
For DGK expression, BMMCs were lysed in 1% NP-40 lysis buffer (1% NP-40, 150 mM NaCl, 50 mM Tris, pH 7.4) with protease inhibitors. Proteins were resolved by SDS-PAGE, transferred to Trans-Blot Nitrocellulose membrane (Bio-Rad Laboratories), and probed with an anti-DGK antibody for DGK expression (71). To analyze Ras, Erk, Mek1/2, Jnk, and PLC1/2 activation, IgE-sensitized BMMCs were resuspended in Tyrode's buffer. Cells were left unstimulated or stimulated with DNP-HSA for different times or PMA (100 ng/ml) for 5 min. For IgE alone activation of Ras and Erk, cells were not sensitized, but rather were stimulated with 1 μg/ml IgE or PMA. Phosphorylation of these proteins was determined by Western blot with antiphospho-specific antibodies for Erk1/2, Mek1/2, Jnk, Akt, and PLC1 and PLC2 (Cell Signal Technology). Membranes were stripped and reprobed with antibodies to Erk, Mek1, Jnk, Akt, and actin for loading controls. Activated Ras in cell lysates was determined by GST-Raf-RBD "pull-down" assay as described previously (38).
PKC membrane localization.
BMMCs were sensitized for 4 h with 1 μg/ml IgE in IMDM-15 without cytokines and rested for 1 h at 37°C in Tyrode's buffer. Cells were stimulated with 50 ng/ml DNP-HSA or 100 ng/ml PMA for 10 min, and membrane fractions were isolated as described previously (72). Protein concentration in Triton soluble fraction was quantified using a bicinchonic acid assay (Pierce Chemical Co.) before PAGE analysis. Western blots were probed with antibodies to PKC (Cell Signal Technology), PKC?II (Santa Cruz Biotechnology, Inc.), and calnexin (Stressgen Bioreagents).
Detection of IL-6 production.
Measurement of IL-6 production by BMMCs was performed as described with modifications (13). BMMCs were rested overnight in IMDM-15 plus IL-3. For the unstimulated condition, cells were resuspended in IMDM-10 at 2.5 x 105 cells/ml. 200 μl cells were seeded in each well of a 96-well plate in triplicate. For FcRI stimulation, cells were washed and sensitized with 1 μg/ml anti-DNP IgE in IMDM-10 at 107 cells/ml for 4 h, pelleted, washed once with IMDM-10, and resuspended at 5 x 105 cells/ml in IMDM-10. 100 μl aliquots of cells were placed into wells of a 96-well plate, followed by addition of 100 μl of IMDM-10 with 2 μg/ml of anti-DNP-IgE, with 60 ng/ml DNP-HSA, or with 40 ng/ml PMA and 200 ng/ml Io. Cells were incubated at 37°C with 5% CO2 for 24 h and IL-6 in supernatants was measured using a murine IL-6 ELISA kit (Pierce Chemical Co.). Data are normalized to PMA/Io control.
?-hexosaminidase release assay.
Hexosaminidase release assay was performed as described previously with modification (13). BMMCs grown in IMDM-15 supplemented with IL-3 were stimulated with IgE at 37°C for 1 h to assess IgE-induced degranulation or were sensitized with 1 μg/ml IgE for 4 h and left unstimulated or stimulated with 10 ng/ml of DNP-HSA or PMA plus Io at 37°C for 1 h. ?-Hexosaminidase activities in the medium and in whole cell lysates were determined using p-nitro-phenyl-N-acetyl-?-D-glucosamide as the substrate.
Passive cutaneous anaphylaxis assay.
The passive cutaneous anaphylaxis assay was performed according to published protocols (73). Mice were anesthetized by intraperitoneal injection of 300 μl of 2.5% 2,2,2-tribromoethanol in tert-amyl alcohol/PBS (1/40; Sigma-Aldrich), followed by subcutaneous injection of 25 ng IgE in 25 μl PBS in the right ear and 25 μl PBS in the left ear. 24 h later, mice were anesthetized and 200 μl antigen (100 μg DNP-HSA, 1% Evans blue in PBS) was injected intravenously via the retroorbital sinus. 30 min after the injection, mice were killed and both ears were removed. Ears were incubated in 200 μl formamide at 55°C for 48 h to extract the dye. Tissue debris was removed by centrifugation and the intensities of the dye were measured by absorption at 610 nm. The data are calculated as OD610 of the IgE-injected ear minus the OD610 of the PBS-injected ear from the same mouse.
Calcium flux.
BMMCs were sensitized with 1 μg/mL IgE for 4 h; resuspended at 107 cells/ml in Tyrode's buffer containing 3 μg/ml Indo-1 (Invitrogen) and 4 mM probencid; and incubated for 30 min at 37°C. Cells were washed twice with Tyrode's buffer and resuspended at 2 x 107 cells/ml. 40 μl of cells was added into 460 μl of prewarmed Tyrode's buffer to measure Ca2+ responses by flow cytometry (BD-LSR; Becton Dickinson). After collection of the baseline ratio of FL5 to FL4, 10 μl of 5 μg/ml DNP-HSA was added to stimulate cells. Calcium flux was assessed as the ratio of FL5 to FL4 fluorescence.
Online supplemental material.
For measurement of DGK transcript levels, RNA was isolated from WT and DGK–/– BMMCs by TRIzol extraction (Invitrogen) and cDNA generated by reverse transcriptions (CLONTECH Laboratories, Inc.). Transcripts were quantified by SYBR green real-time PCR using the following primers: DGK: 5'-GATGCAGGCACCCTGTACAAT-3', 5'-GGACCCATAAGCATAGGCATCT-3'; DGK: 5'-GGGACCTCAAGGACCTTGGT-3', 5'-TCAGCTCCTTGATCCCACAAA; and DGK: 5'-TTCCCCAGGGCACTCTCA-3', 5'-CAGACGTTGCATCTAGGAAGCA-3'. No products were amplified from a no reverse transcriptase control sample (unpublished data). Transcripts were normalized to GAPDH signal (5'-GAAGGTACGGAGTCAACGGATTT-3', 5'-GAATTTGACCATGGGTGGAAT-3') using the Ct method. For measurement of total cellular protein levels of PKC?II and PKC, WT and DGK–/– BMMCs were left unstimulated for 4 h in cytokine-free media with or without IgE (1 μg/ml). Cells were lysed in 1% NP-40 lysis buffer with protease inhibitors, proteins were resolved by SDS-PAGE, and Western blots were probed with antibodies to PKC?II or PKC. Blots were stripped and reprobed for actin as a loading control. Online supplemental material is available at http://www.jem.org/cgi/content/full/jem.20052424/DC1.
Acknowledgments
We thank J. Stadanlick for help in preparation of the manuscript; M. Jordan for help in the Ca++ experiment; S. Prescott and M. Topham for providing the anti-DGK antibody; E. Myers and E. Hainey for technical assistance; and Drs. Q.-C. Yu, H.-W. Yu, and Y. Wang for assistance in histological analysis.
This work was supported by the National Institutes of Health (G.A. Koretzky and X.-P. Zhong), from the Sandler Program for Asthma Research (G.A. Koretzky), and from the National Cancer Institute (B.A. Olenchock).
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3 Department of Pediatrics and 4 Department of Immunology, Duke University Medical Center, Durham, NC 27710
CORRESPONDENCE Gary Koretzky: koretzky@mail.med.upenn.edu OR Xiao-Ping Zhong: zhong001@mc.duke.edu
Calcium and diacylglycerol are critical second messengers that together effect mast cell degranulation after allergen cross-linking of immunoglobulin (Ig)E-bound FcRI. Diacylglycerol kinase (DGK) is a negative regulator of diacylglycerol-dependent signaling that acts by converting diacylglycerol to phosphatidic acid. We reported previously that DGK–/– mice have enhanced in vivo T cell function. Here, we demonstrate that these mice have diminished in vivo mast cell function, as revealed by impaired local anaphylactic responses. Concordantly, DGK–/– bone marrow–derived mast cells (BMMCs) demonstrate impaired degranulation after FcRI cross-linking, associated with diminished phospholipase C activity, calcium flux, and protein kinase C–?II membrane recruitment. In contrast, Ras-Erk signals and interleukin-6 production are enhanced, both during IgE sensitization and after antigen cross-linking of FcRI. Our data demonstrate dissociation between cytokine production and degranulation in mast cells and reveal the importance of DGK activity during IgE sensitization for proper attenuation of FcRI signals.
Abbreviations used: BMMC, bone marrow–derived cell; DAG, diacylglycerol; DGK, DAG kinase; IP3, inositol 1,4,5-trisphosphate; LAT, linker for activated T cells; MAPK, mitogen-activated protein kinase; PA, phosphatidic acid; PCA, passive cutaneous anaphylaxis; PI5K, phosphatidylinositol 4-phosphate 5-kinase; PIP2, phosphatidylinositol 4,5-bisphosphate; PKC, protein kinase C; PLC, phospholipase C.
B.A. Olenchock and R. Guo contributed equally to this work.
Mast cells play important roles in both innate and adaptive immune responses. They are central effector cells in immune responses to parasites and in the pathogenesis of diseases such as asthma and allergy (1, 2). The high affinity receptor for IgE (FcRI) is one of several cell surface receptors critical for mast cell development and function (3). FcRI binds to IgE in the absence of antigen and subsequent cross-linking of IgE-bound FcRI by cognate antigen induces a signaling cascade that leads to mast cell degranulation and cytokine secretion, which contribute to both chronic allergic inflammation and acute anaphylaxis. Understanding FcRI signaling and mast cell activation is critical to devising new therapies for mast cell–mediated diseases.
Recent studies have greatly improved our understanding of FcRI signaling. After FcRI engagement, the Src family members Lyn and Fyn and the tyrosine kinase Syk are activated (4, 5). These molecules in turn recruit and activate other kinases such as the Tec family kinase Btk (6), phospholipid modifying enzymes including phosphatidylinositol 4,5-bisphosphate 3-kinase (PI3K) (7), the GTPase-activating molecule Vav1 (8), and adaptor molecules such as linker for activated T cells (LAT) (9), non– T cell activation linker (NTAL/LAB) (10, 11), SH2 domain containing leukocyte phosphoprotein of 76 kD (SLP-76) (12, 13), and Grb2-associated binder protein 2 (Gab2) (14). The formation of a multimolecular signaling complex coordinates activation of various downstream signaling pathways necessary for mast cell effector functions. These pathways include phospholipase C (PLC) (15, 16), protein kinase C (PKC) isoforms (17, 18), and mitogen-activated protein kinases (MAPKs) (19). PLC hydrolyzes the membrane phospholipid phosphatidylinositol 4,5-bisphosphate (PIP2), leading to the generation of two important second messengers, diacylglycerol (DAG) and inositol 1,4,5-trisphosphate (IP3). IP3 binds to its receptor in the endoplasmic reticulum and induces Ca2+ release into the cytoplasm. DAG recruits to the membrane and activates PKC family members and RasGRPs, which are recently identified guanine nucleotide exchange factors for Ras and Rap (20). Synergistic action of multiple downstream signals, particularly Ca2+ and PKCs, are required to induce mast cell degranulation (18, 21, 22). Activated PKCs and MAPKs together promote transcription of many proinflammatory genes, including cytokines (22–25).
Both in vitro and in vivo evidence suggest a critical role for DAG in the regulation of mast cell function after FcRI engagement. Treatment of mast cells with DAG analogues in the presence of a Ca2+ ionophore can mimic FcRI engagement and induce mast cells to degranulate and release active mediators (26, 27). Mice lacking PLC2, the enzyme that generates IP3 and DAG, have diminished mast cell function (28, 29). Similarly, deficiency in DAG effector molecules alters mast cell function. Multiple PKCs are expressed in mast cells, and activation of both classical and novel isoforms of PKC is regulated by DAG (18, 30). Different PKCs have distinct functions in mast cells. PKC?–/– mast cells demonstrate decreased IL-6 production and degranulation in response to FcRI engagement (22), whereas PKC–/– mast cells respond more vigorously to suboptimal FcRI stimulation with more sustained Ca2+ mobilization and increased degranulation compared with WT mast cells (31). Thus, proper balance of PKC? and PKC activities appears important for mast cell function.
These observations suggest that DAG levels must be tightly controlled in mast cells. One mechanism for terminating DAG signaling is by phosphorylation catalyzed by the DAG kinase (DGK) family of enzymes. Phosphorylation of DAG by DGKs converts DAG to phosphatidic acid (PA), thus preventing DAG from activating PKCs and RasGRPs (20, 32–34). Additionally, PA itself is a second messenger, and DGK activity could regulate mast cell function by affecting PA accumulation. In vitro, PA is a potent activator of PLC and phosphatidylinositol 4-phosphate 5-kinase (PI5K), enzymes involved in PIP2 degradation and production (35–37). Therefore, through conversion of DAG into PA, DGK enzymes could regulate many aspects of inositol lipid metabolism and mast cell activation after FcRI engagement.
We recently described mice deficient in DGK and demonstrated that T cells from these animals are hyper-responsive to TCR stimulation. DGK–/– mice mount enhanced antiviral immune responses, indicating that DGK is an important in vivo negative regulator of TCR signaling and T cell activation (38, 39). We show here that DGK also regulates immune receptor signaling in mast cells. To our surprise, in vivo mast cell function is impaired in DGK–/– mice as indicated by diminished local anaphylactic responses. To explore the mechanism underlying this finding, we have studied DGK–/– bone marrow–derived mast cells (BMMCs). We demonstrate that FcRI-induced degranulation of DGK–/– BMMCs is diminished, correlating with impaired PLC activation and PKC?II membrane translocation. Similar to what we have observed after TCR stimulation, however, FcRI-induced activation of the Ras–Erk signaling pathway is enhanced and DGK–/– BMMCs produce increased IL-6 during IgE sensitization and after antigen cross-linking of the FcRI. Moreover, mast cell survival after growth factor withdrawal is greatly increased by DGK deficiency, correlating with maintained phosphorylation of Akt. These findings indicate that DGK functions to maintain mast cell responsiveness to antigen stimulation during passive sensitization with IgE and demonstrate separation of cytokine production and degranulation after FcRI stimulation of mast cells.
RESULTS
Mast cells develop in DGK-deficient mice
We previously reported that DGK plays an important role in T cell activation (38, 39). DGK is also expressed in mast cells and, as in T cells, the 115-kD isoform is prominent (Fig. 1 A ). There are also smaller species reactive with the anti-DGK antibody, which may be products of protein degradation, as mast cells are rich in granules containing proteases. Alternatively, these might represent products of alternate transcripts. Importantly, the three major species reactive with the DGK antibody are all absent in BMMCs from targeted mice (Fig. 1 A). Mast cell development is unaffected by DGK deficiency for the following reasons: the numbers of mast cells in ear, skin, stomach, and spleen are similar in WT and DGK–/– mice (Fig. 1 B and not depicted); electron microscopy did not reveal any differences in cell morphology or number of intracellular granules (not depicted); and KO mast cells express similar levels of c-Kit and FcRI on their surfaces (Fig. 1 C). Additionally, DGK deficiency does not result in compensatory up-regulation of transcripts for related DGK isoforms (Fig. S1, available at http://www.jem.org/cgi/content/full/jem.20052424/DC1).
Figure 1. DGK expression and surface expression of FcRI and c-Kit in BMMCs from WT and DGK-deficient mice. (A) DGK protein in cell lysates made from WT and DGK-deficient BMMCs was detected by Western blot analysis using an antibody specific for the carboxyl-terminus of DGK (reference 71). The arrow indicates the 115-kD 1 isoform. (B) Mast cell distribution in the skin. Mast cells in the skin (back) and ears were stained with toluidine blue and were counted under a light microscope. Data shown are the means ± standard error of the number of mast cells per high-power field (10 x 100). (C) FcRI and c-Kit expression on BMMCs. For FcRI expression, WT and DGK-deficient BMMCs were incubated with 1 μg/ml anti-DNP IgE for 4 h (solid line) and FcRI expression was detected by staining with a FITC-labeled anti-IgE secondary antibody. Cells that had not been incubated with IgE serve as a control (dotted line). For c-Kit expression, WT and DGK-deficient BMMCs were either stained with a PE-labeled control antibody (dotted line) or a PE-labeled anti–c-Kit antibody (solid line).
Decreased passive cutaneous anaphylaxis in DGK-deficient mice
DGK–/– T cells have enhanced homeostatic proliferation and antiviral responses in vivo (39). To test the importance of DGK in mast cell function, we assessed allergic responses by examining passive cutaneous anaphylaxis (PCA), an in vivo measure of FcRI-dependent mast cell function. Unexpectedly, DGK–/– mice had significantly impaired localized anaphylactic responses (Fig. 2 A ).
Figure 2. Decreased passive cutaneous anaphylaxis and FcRI-induced degranulation but increased IL-6 production as the result of DGK deficiency. (A) WT and DGK–/– mice were injected subcutaneously with 25 ng IgE in 25 μl PBS in the right ear and with 25 μl PBS in the left ear. 24 h later, DNP-HSA and Evans blue dye were injected intravenously into the mice. 30 min after injection, tissue from the ears was collected, Evans blue was extracted, and the intensity of the dye was measured by absorption at 610 nm (OD610). Each data point is OD610 of IgE-injected ear minus the OD610 of PBS-injected ear from the same mouse. Data shown comprise three experiments. (B) Decreased FcRI-induced degranulation in DGK–/– BMMCs. IgE-sensitized WT and DGK–/– BMMCs were left unstimulated or were stimulated with various concentrations of DNP-HSA at 37°C for 60 min. Cells were spun, and ?-hexosaminidase activities in supernatants as well as in whole cell lysates of unstimulated BMMCs were measured. Data were calculated as percentage of ?-hexosaminidase activity in the supernatant to the activity in the whole cell lysates of the same genotype. Means ± standard error of triplicates are shown. Data are representative of three experiments. (C) Increased IL-6 production in DGK-deficient BMMCs. WT and DGK-deficient BMMCs were left unstimulated, were stimulated with 1 μg/ml IgE overnight, or were sensitized with 1 μg/ml IgE for 4 h and cross-linked with 30 ng/ml DNP-HSA overnight. IL-6 in the culture medium was measure by ELISA. Data shown are means ± standard error of triplicates normalized to PMA/Io control and are representative of three experiments.
To explore why DGK–/– mice demonstrate impaired PCA responses, we first compared FcRI-triggered degranulation in WT versus DGK–/– BMMCs by measuring ?-hexosaminidase release (Fig. 2 B). FcRI-induced degranulation was significantly diminished in DGK–/– BMMCs (Fig. 2 B). PMA plus ionomycin (Io) stimulation, however, resulted in similar degranulation in WT and DGK–/– BMMCs, indicating that the ability to release granules and total granule content is unaffected by DGK deficiency. The impairment of FcRI-induced mast cell degranulation likely contributes to the decreased PCA responses in DGK–/– mice.
Another consequence of FcRI engagement is the production of proinflammatory cytokines such as IL-6. IgE alone can induce a significant amount of IL-6 production in WT BMMCs (Fig. 2 C), which is consistent with previous reports (40). Cross-linking the receptor with antigen induces even more IL-6 production. Under both stimulation conditions, DGK–/– BMMCs produce approximately twofold more IL-6 than WT BMMCs. Therefore, DGK deficiency impairs FcRI-induced degranulation, but increases cytokine production after IgE sensitization and after cross-linking of the receptor with antigen.
Antigen stimulation of IgE-sensitized BMMCs
Cross-linking of IgE-bound FcRI results in activation of a signaling network that coordinates mast cell effector functions. To investigate why DGK–/– BMMCs have impaired degranulation but enhanced cytokine production after FcRI stimulation, we assessed how DGK deficiency affects antigen-induced FcRI signaling in IgE-sensitized BMMCs. We first verified that DGK phosphorylates DAG after antigen stimulation of BMMCs by measuring PA production. Addition of DNP-HSA to IgE-sensitized WT BMMCs results in robust PA accumulation beginning 5–10 min after stimulation (Fig. 3 A ). As expected, antigen stimulation of DGK–/– BMMCs results in significantly less PA accumulation.
Figure 3. Antigen stimulation of IgE-sensitized BMMCs. (A) DGK deficiency impairs PA production by BMMCs after FcRI stimulation. BMMCs were sensitized for 4 h with IgE, labeled with 32P-orthorphosphate, and either left unstimulated or stimulated with 10 ng/ml DNP-HSA for 10 min. Lipids were extracted, separated by TLC, and quantified using a phosphorimager. PA, the product of DAG phosphorylation, was identified by comigration with a standard. Data are presented as fold-induction calculated by cpm of stimulated cells divided by cpm of unstimulated cells. Means ± standard error of four experiments are shown; *, P < 0.05. (B–D) WT and DGK–/– BMMCs were sensitized with IgE for 4 h and left unstimulated (U) or were stimulated either with 4 ng/ml of DNP-HSA for different times or with 100 ng/ml PMA (P) for 5 min. (B) AKT phosphorylation was assessed by immunoblot analysis using an antibody specific for phosphorylated Ser473 of Akt. Total Akt is shown as a loading control. (C) Active Ras in lysates was measured by affinity precipitation using GST-Raf-RBD agarose beads followed by immunoblot analysis. (D) MEK1/2 and ERK1/2 activity was assessed by immunoblot analysis using phospho-specific antibodies. Total MEK1/2 and ERK1/2 serve as loading controls. (E) Membrane recruitment of PKC?II is diminished in DGK–/– BMMCs. IgE-sensitized BMMCs were left unstimulated (–) or were stimulated with 50 ng/ml DNP-HSA (DNP) or PMA (P) for 10 min. Triton-soluble membrane fractions were prepared and membrane translocation of PKC isoforms was determined by Western blot using antibodies to PKC?II, PKC, and calnexin (CNX) as a loading control. One representative blot is shown and data from five (PKC?II) or three (PKC) experiments were quantified and normalized to CNX; combined data are represented graphically.
We next examined signaling pathways that have been implicated in cytokine production after FcRI ligation. Activation of the PI3K/Akt and Ras/Erk pathways is required for cytokine production (23, 25, 41). Low dose stimulation of IgE-sensitized WT BMMCs with DNP-HSA weakly activates Akt, but stimulation of DGK–/– BMMCs results in significantly increased Akt activation (Fig. 3 B). FcRI activation of Ras is believed to be the result of Grb2-SOS activation (42, 43), but recent reports suggest that DAG might contribute to Ras activation through allosteric activation of the Ras guanine-nucleotide exchange factor RasGRP4 (44–46). As shown in Fig. 3 C, FcRI-induced Ras activity is enhanced in DGK–/– BMMCs. Consistent with the increased Ras activation, we observed enhanced and prolonged Mek1/2 and Erk1/2 phosphorylation in DGK–/– BMMCs compared with WT BMMCs (Fig. 3 D). The effect of DGK deficiency is selective, however, as FcRI-induced activation of the MAPKs p38 and Jnk is similar in WT and DGK–/– BMMCs (unpublished data). These data demonstrate that DGK deficiency enhances FcRI-induced activation of Akt, Ras, and Erk1/2, likely contributing to enhanced cytokine production.
Activation of PKC family members by DAG and Ca2+ coordinates mast cell degranulation after FcRI stimulation (22, 47). As expected, antigen cross-linking induces membrane recruitment of PKC?II and PKC in WT BMMCs (Fig. 3 E). However, we find that membrane recruitment of PKC?II is clearly diminished in DGK–/– BMMCs, whereas PKC recruitment is preserved. Unstimulated IgE-sensitized DGK–/– BMMCs also demonstrate diminished levels of membrane-associated PKC?II but normal PKC levels. Moreover, treatment with the DAG analogue PMA, which is not a DGK substrate and should be unaffected by DGK deficiency, results in impaired movement of PKC?II to the membrane in DGK–/– BMMCs but normal movement of PKC (Fig. 3 E, representative blot and graphical summary of replicates). The block in PKC?II recruitment was not the result of diminished protein levels, however, as total levels of PKC?II and PKC in whole cell lysates were not decreased in DGK–/– BMMCs as compared with WT BMMCs (Fig. S2, available at http://www.jem.org/cgi/content/full/jem.20052424/DC1). These data provide a likely mechanism for the impaired degranulation we observe in DGK–/– BMMCs, as FcRI cross-linking results in less recruitment of a positive regulator (PKC?II) of mast cell degranulation, but appropriate recruitment of a negative regulator of mast cell degranulation (PKC). The data also suggest that DGK is essential for FcRI activity in addition to its effect on DAG levels, as PMA and PMA/Io (unpublished data) fail to restore PKC?II recruitment in DGK–/– BMMCs.
Calcium response and PLC activity in DGK–/– BMMCs
The diminished membrane recruitment of the Ca2+-dependent PKC?II along with the preserved movement of the Ca2+-independent PKC led us to question whether DGK deficiency affects FcRI-induced Ca2+ flux. Compared with WT BMMCs, DGK–/– BMMCs have a significantly diminished Ca2+ response after FcRI stimulation by antigen (Fig. 4 A ). Consistent with the decreased Ca2+ response, phosphorylation of PLC1 and PLC2 after stimulation of the FcRI was decreased in DGK–/– BMMCs (Fig. 4 B). As tyrosine phosphorylation of PLC does not always correlate with its enzymatic activity (48), we analyzed PLC activity by assessing metabolism of the PLC substrate PIP2 and production of IP3. After receptor cross-linking in WT BMMCs, PIP2 levels quickly decrease (Fig. 4 C), and IP3 levels increase (Fig. 4 D) as a result of PLC activity. Upon stimulation of DGK–/– BMMCs, we do not observe a decrease but rather a slight increase in PIP2 levels (Fig. 4 C), and IP3 generation is impaired (Fig. 4 D). These data provide compelling evidence that DGK deficiency impairs activation of PLC after antigen stimulation of IgE-sensitized mast cells.
Figure 4. Decreased Ca2+ responses and PLC activity in DGK–/– mast cells. WT and DGK–/– BMMCs were sensitized for 4 h with IgE in cytokine-free media. (A) Deceased Ca2+ flux in DGK–/– mast cells after FcRI stimulation. WT and DGK–/– BMMCs were loaded with Indo-1 and stimulated with 100 ng/ml DNP-HSA to induce Ca2+ responses. Ca2+ flux was determined by flow cytometry based on the change of FL5/FL4 ratio. Data shown are representative of four experiments. (B) Decreased PLC phosphorylation in DGK–/– BMMCs after FcRI stimulation. BMMCs were stimulated with different concentrations of DNP-HSA for 2 min. PLC phosphorylation was determined by Western blot with anti–phospho- PLC1 and anti–phospho-PLC2 antibodies. The blots were probed with an anti-actin antibody as a loading control. (C) Decreased PIP2 hydrolysis in DGK–/– BMMCs. Cells were labeled with 32P-orthophosphate and stimulated for the indicated amounts of time with 10 ng/ml DNP-HSA; lipids were analyzed as in Fig. 3. PIP2 was identified by comigration with a standard. Data are means ± standard error of four different experiments. *, P = 0.01, 0.5 min stimulation, WT vs. DGK KO. (D) Diminished IP3 generation in DGK–/– BMMCs. Cells were left unstimulated or were stimulated with 10 ng/ml DNP-HSA for 20 s or 2 min and lysed using perchloric acid, and IP3 was measured.
IgE signaling and function in the absence of antigen
IgE sensitization of DGK–/– BMMCs leads to increased cytokine production and impaired PKC?II recruitment to the membrane, so we therefore examined how IgE alone signaling and function is altered in DGK deficiency. IgE binding to FcRI induces a large increase in PA in WT BMMCs (Fig. 5 A ). DGK–/– BMMCs, in contrast, have a significant impairment in PA accumulation during IgE sensitization. DAG-dependent signaling is also enhanced in DGK–/– BMMCs during IgE sensitization, as Ras and Erk1/2 activity is enhanced (Fig. 5 B).
Figure 5. IgE stimulation in the absence of antigen cross-linking results in enhanced signaling in DGK–/– BMMCs. BMMCs were rested in media without cytokines for at least 4 h and rested for 1 h in Tyrode's buffer before stimulation. (A) Impaired PA production in DGK–/– BMMCs. Cells were labeled with 32P-orthophosphate for 1 h and stimulated with 1 μg/ml IgE for 30 min. Lipids were extracted and PA production was quantified as in Fig. 3. Means ± standard error of five experiments are shown. *, P < 0.05. (B) Enhanced Ras/ERK activation in DGK–/– BMMCs. BMMCs were stimulated with 1 μg/ml IgE for various amounts of time or with 100 ng/ml PMA for 5 min. Active Ras and ERK1/2 phosphorylation were assessed as in Fig. 3. For the Ras blot, a space is included before the PMA lanes to designate that these samples were run on a separate gel.
IgE binding to the FcRI signals mast cell survival through up-regulation of antiapoptotic proteins (40, 49–52), and ex vivo mast cell survival and expansion requires IL-3 (53, 54). In the presence of IL-3, both WT and DGK–/– mast cells survive and expand similarly (unpublished data). When IL-3 is withdrawn, WT BMMCs undergo apoptosis as expected (Fig. 6 A ). Surprisingly, DGK–/– BMMCs have greatly enhanced survival in the absence of IL-3. IgE enhances survival in both WT and DGK–/– BMMCs, but because survival in the absence of cytokines is so much greater in the DGK–/– BMMCs, the IgE survival effect is less marked (Fig. 6, A and B).
Figure 6. Enhanced survival of DGK–/– BMMCs after IL-3 withdrawal. WT and DGK–/– BMMCs were cultured in media without cytokines in the presence of different concentrations of IgE for 48 or 110 h. Survival of BMMCs was determined by staining with FITC-annexin V and PI and analyzed by flow cytometry. (A) Representative dot-plots. (B) Percentage of live cells (Annexin-V and PI negative) in a full time course and at a range of concentrations of IgE. Data shown are representative of three experiments. (C) Akt phosphorylation during growth in cytokine-replete media (+IL3/SCF) and after 18 h cytokine withdrawal (18 h, no cytokines) was assessed by immunoblot analysis. One representative blot is shown and data from three independent experiments were quantified, normalized to PLC1 signal, and represented graphically for comparison. P-AKT signal in WT cells grown in cytokine-replete media was arbitrarily set to 1.
Akt regulates cell survival and is activated by IgE binding to FcRI (40). Akt is phosphorylated in WT BMMCs grown in cytokine-replete media, and this activation decreases after withdrawal of cytokines (Fig. 6 C). DGK–/– BMMCs, in contrast, have enhanced Akt activity during growth in cytokine-replete media and maintain Akt activity after cytokine removal (Fig. 6 C). As cytokines stimulate inositol metabolism, including PIP2 hydrolysis by PLC and phosphorylation by PI3K (55, 56), it is likely that DGK regulates signals generated through cytokine receptors in addition to its role in FcRI signaling. Future work will explore the biochemical basis of this observation.
DISCUSSION
We have studied mice that lack a key enzyme involved in DAG metabolism, DGK, to address the consequences of dysregulated DAG accumulation after immune receptor signaling. We demonstrated recently that DGK functions as a key negative regulator of TCR signaling and T cell activation (38, 39). We show here that DGK plays an important and unexpected role in regulating signal transduction from the FcRI in mast cells. DGK–/– BMMCs manifest decreased PA production, enhanced activation of the Ras-Mek-Erk signaling pathway, increased Akt phosphorylation, prolonged survival after cytokine deprivation, and enhanced production of IL-6 as compared with WT BMMCs. Surprisingly, IgE-mediated PCA responses are significantly decreased in DGK–/– mice, concordant with impairment of receptor-induced PLC activity and degranulation in DGK–/– BMMCs. We demonstrate that signals generated by IgE in the absence of antigen cross-linking are enhanced in DGK–/– BMMCs. These data demonstrate that DGK is important for inactivation of DAG-mediated signaling pathways in mast cells and that DGK also plays a critical role in maintaining FcRI responsiveness to antigen cross-linking. In addition, we demonstrate a novel FcRI signaling alteration in DGK–/– BMMCs, in that receptor engagement results in poor PLC activity and degranulation but augmented cytokine production.
The observation that DGK deficiency impairs PLC function after FcRI stimulation of mast cells was unexpected, as DGK was predicted to function downstream of PLC. It is possible that enhanced DAG-dependent signaling during IgE sensitization of DGK–/– BMMCs promotes feedback inhibition of PLC and Ca2+ responses upon antigen cross-linking of the FcRI. Short pretreatment of mast cells with phorbol esters results in feedback inhibition of PLC that is mediated by PKC and PKC (57–59). Prolonged administration of phorbol esters, in contrast, down-regulates PKC isoforms and potentiates PLC activity upon antigen stimulation (59). We do not see changes in PKC protein levels in DGK–/– BMMCs, and we report impaired PLC activity. PKC feedback inhibition might be indirect as well, as PKC? can induce serine-phosphorylation of Btk at an inhibitory site, dampening Btk activation in mast cells (60). Btk phosphorylates and activates PLC after FcRI stimulation, so feedback inhibition of Btk could contribute to diminished PLC activity (61). Alternatively, enhanced Erk activation in DGK–/– BMMCs could inhibit PLC association with LAT, as has been observed in T cells after TCR engagement (62). However, we have not observed an obvious decrease in PLC2-LAT association in DGK–/– BMMCs after antigen cross-linking of the FcRI (unpublished data).
Alternatively, diminished PLC activity and PKC?II membrane recruitment might be a direct consequence of DGK deficiency. Although DGK activity terminates DAG signaling, it also creates PA (32, 33, 63). PA is a potent activator of PLC enzymatic activity in vitro (35). In addition, a recent report suggests that DGK, through production of PA, may increase intracellular PIP2 by activation of PI5K I (37). Thus, DGK deficiency could lead to decreased PI5K activity, diminishing levels of the PLC substrate PIP2. Our PIP2 measurements did not reveal any differences in 32P incorporation into PIP2 in IgE-sensitized BMMCs (unpublished data), but more direct measures of PIP2 mass should be performed to ensure that steady state levels of 32P-labeled PIP2 reflect total mass. The importance of diminished PA production to the phenotype of DGK–/– BMMCs is particularly difficult to assess, as alternative pathways to generate PA exist. These pathways include the hydrolysis of phosphatidylcholine mediated by phospholipase D and the acylation of lyso-PA by lyso-PA acyltransferases (63). phospholipase D–derived PA has been reported to regulate diverse cellular processes, particularly in vesicle transportation and exocytosis (64, 65). It is possible that PA generated by DGK performs a similar function to promote mast cell degranulation.
It is intriguing that membrane recruitment of PKC?II is diminished in unstimulated IgE-sensitized DGK–/– BMMCs and that PKC?II recruitment is not restored with PMA treatment. PMA is a DAG analogue and is not subject to phosphorylation by DGK, so we predict that if DGK acts only by regulating DAG levels, PMA treatment should restore PKC?II membrane recruitment. It is possible that DGK has adaptor functions in addition to its role in lipid metabolism, perhaps by participating in a complex with PKC?II or Btk directly (37, 66). Future work will explore this interesting observation.
We have been unable to directly measure an FcRI- induced change in DAG mass in WT or DGK–/– mast cells using standard biochemical approaches (unpublished data). The likely explanation is that the receptor-induced pool of DAG is a small fraction of the total cellular pool because DAG is important for other aspects of cell biology. We are currently developing imaging approaches to measure DAG localization using a fluorescently labeled DAG probe (67). We also will develop HPLC/MS/MS techniques to quantify particular DAG subspecies, which may be more markedly regulated than total cellular DAG (68). These approaches will allow us to measure dynamic changes in DAG localization after FcRI stimulation as well as assess in vivo substrate specificity of DGK.
The increased Akt phosphorylation in DGK–/– BMMCs stimulated through cytokine or FcRs is intriguing. It is possible that increased Akt activity is a consequence of greater PIP3 production in DGK–/– BMMCs, and preliminary data support this hypothesis. Decreased PA production in DGK–/– BMMCs might increase PI3K activity, as PA has been reported to inhibit this enzyme in vitro (69). Also, perhaps decreased PLC activity in DGK–/– BMMCs increases the local concentration of PIP2 available as substrate for PI3K (66). The interrelation among different PI metabolites is complex and understanding the exact lipid alterations will require further study.
Our current studies of DGK in mast cells reveal important roles for this enzyme in regulating FcRI signaling. DGK is not only essential for terminating DAG activity but also appears to be critical for maintaining optimal FcRI responsiveness to antigen cross-linking. A more complete understanding of the importance of DGK activity to mast cell function requires analysis of other DGK family members. Ongoing biochemical and genetic studies are addressing this question.
MATERIALS AND METHODS
DGK-deficient mice.
DGK–/– mice have been described previously (39) and were housed in pathogen-free facilities at the University of Pennsylvania and Duke University. All experiments using animals were performed in accordance with regulations of the Institutional Animal Care and Use Committee of the University of Pennsylvania and Duke University.
Microscopic analysis of mast cells.
Skin samples from the back of the trunk and the ears were collected from killed WT and DGK–/– mice. Tissues were fixed and mounted in paraffin according to standard histological procedures. Paraffin sections were stained with toluidine blue and mast cells in tissues were evaluated by microscopy. In each tissue, mast cells were counted in 10 contiguous high-power fields (10 x 100).
BMMCs.
BM cells from tibias and femurs from WT and DGK–/– mice were harvested and incubated with Isocove's medium (Mediatech, Inc.) supplemented with 15% FBS (Hyclone), 100 U/ml penicillin G, 100 U/ml streptomycin, and 292 μg/ml of L-glutamine, 10 mM Hepes (pH 7.4), 0.1 mM nonessential amino acid, 1 mM sodium pyruvate, and 50 μM 2-mercaptoethanol (IMDM-15) with IL-3–conditioned medium for 2 wk and further expanded for an additional 2–8 wk with the supplement of SCF-conditioned medium made from cell lines engineered to produce these cytokines (70).
Flow cytometry.
BMMCs were analyzed directly or after 4-h sensitization with 1 μg/ml IgE. Cells were stained with fluorescently labeled antibodies in 5% FBS in PBS and were analyzed on a FACSCaliber (Becton Dickinson) with CELLQuest software. Antibodies used were PE-conjugated c-Kit and FITC-conjugated anti-IgE (BD Biosciences). To measure cell survival after cytokine withdrawal, cells were stimulated in IMDM-15 without cytokine at a concentration of 106 cells/ml in a 96-well plate with different concentrations of anti-DNP–IgE (0, 0.04, 0.2, 1, or 5 μg/ml; Sigma-Aldrich). After 48 or 110 h incubation, cells were stained with propidium iodide and annexin V–FITC (BD Biosciences) and were analyzed by flow cytometry.
Measurement of PA and PIP2.
BMMCs were sensitized at 37°C for 4 h in 1 μg/ml IgE in IMDM-15 without IL-3 or SCF. Cells were harvested and rested in Tyrode's buffer (10 mM Hepes, pH 7.4, 130 mM NaCl, 1 mM MgCl2, 5 mM KCl, 1.4 mM CaCl2, 5.6 mM glucose, and 1 mg/ml bovine serum albumin) for 1 h at 37°C. 32P-phosphoric acid (MP Biomedicals) was added to a concentration of 0.25 mCi/ml. Cells were left unstimulated or were stimulated with 10 ng/ml DNP-HSA. Stimulation was terminated by addition of 0.1 volume of ice-cold 2 M HCl and transfer of cells to ice for 10 min. Lipids were extracted with 3 ml of 2:1 methanol:chloroform and phases were separated by addition of 2 ml 1 N NaCl and 2 ml of chloroform. Lipid phase was washed 1x with 3 ml of upper phase buffer (upper phase of 10:10:9 chloroform:methanol:1 M NaCl), dried under nitrogen, and separated by thin-layer chromatography using a basic solvent (9:7:2 chloroform: methanol: 4 M NH4OH). PA and PIP2 were identified by comigration with standards (Sigma-Aldrich) and quantified using a phosphorimager.
Measurement of IP3.
IgE-sensitized BMMCs were rested for 1 h in Tyrode's buffer, then left unstimulated or stimulated for 20 s or 2 min with 10 ng/ml DNP-HSA. Stimulations were terminated by addition of 0.2 vol 20% perchloric acid for 20 min on ice. Proteins were sedimented and supernatants were neutralized to pH 7.5 by titration of 1.5 M KOH 60 mM Hepes containing universal indicator dye (Sigma-Aldrich). KClO4 was precipitated by centrifugation and IP3 was measured in supernatants by radioreceptor assay according to the manufacturer's protocol (PerkinElmer).
Western blot analysis.
For DGK expression, BMMCs were lysed in 1% NP-40 lysis buffer (1% NP-40, 150 mM NaCl, 50 mM Tris, pH 7.4) with protease inhibitors. Proteins were resolved by SDS-PAGE, transferred to Trans-Blot Nitrocellulose membrane (Bio-Rad Laboratories), and probed with an anti-DGK antibody for DGK expression (71). To analyze Ras, Erk, Mek1/2, Jnk, and PLC1/2 activation, IgE-sensitized BMMCs were resuspended in Tyrode's buffer. Cells were left unstimulated or stimulated with DNP-HSA for different times or PMA (100 ng/ml) for 5 min. For IgE alone activation of Ras and Erk, cells were not sensitized, but rather were stimulated with 1 μg/ml IgE or PMA. Phosphorylation of these proteins was determined by Western blot with antiphospho-specific antibodies for Erk1/2, Mek1/2, Jnk, Akt, and PLC1 and PLC2 (Cell Signal Technology). Membranes were stripped and reprobed with antibodies to Erk, Mek1, Jnk, Akt, and actin for loading controls. Activated Ras in cell lysates was determined by GST-Raf-RBD "pull-down" assay as described previously (38).
PKC membrane localization.
BMMCs were sensitized for 4 h with 1 μg/ml IgE in IMDM-15 without cytokines and rested for 1 h at 37°C in Tyrode's buffer. Cells were stimulated with 50 ng/ml DNP-HSA or 100 ng/ml PMA for 10 min, and membrane fractions were isolated as described previously (72). Protein concentration in Triton soluble fraction was quantified using a bicinchonic acid assay (Pierce Chemical Co.) before PAGE analysis. Western blots were probed with antibodies to PKC (Cell Signal Technology), PKC?II (Santa Cruz Biotechnology, Inc.), and calnexin (Stressgen Bioreagents).
Detection of IL-6 production.
Measurement of IL-6 production by BMMCs was performed as described with modifications (13). BMMCs were rested overnight in IMDM-15 plus IL-3. For the unstimulated condition, cells were resuspended in IMDM-10 at 2.5 x 105 cells/ml. 200 μl cells were seeded in each well of a 96-well plate in triplicate. For FcRI stimulation, cells were washed and sensitized with 1 μg/ml anti-DNP IgE in IMDM-10 at 107 cells/ml for 4 h, pelleted, washed once with IMDM-10, and resuspended at 5 x 105 cells/ml in IMDM-10. 100 μl aliquots of cells were placed into wells of a 96-well plate, followed by addition of 100 μl of IMDM-10 with 2 μg/ml of anti-DNP-IgE, with 60 ng/ml DNP-HSA, or with 40 ng/ml PMA and 200 ng/ml Io. Cells were incubated at 37°C with 5% CO2 for 24 h and IL-6 in supernatants was measured using a murine IL-6 ELISA kit (Pierce Chemical Co.). Data are normalized to PMA/Io control.
?-hexosaminidase release assay.
Hexosaminidase release assay was performed as described previously with modification (13). BMMCs grown in IMDM-15 supplemented with IL-3 were stimulated with IgE at 37°C for 1 h to assess IgE-induced degranulation or were sensitized with 1 μg/ml IgE for 4 h and left unstimulated or stimulated with 10 ng/ml of DNP-HSA or PMA plus Io at 37°C for 1 h. ?-Hexosaminidase activities in the medium and in whole cell lysates were determined using p-nitro-phenyl-N-acetyl-?-D-glucosamide as the substrate.
Passive cutaneous anaphylaxis assay.
The passive cutaneous anaphylaxis assay was performed according to published protocols (73). Mice were anesthetized by intraperitoneal injection of 300 μl of 2.5% 2,2,2-tribromoethanol in tert-amyl alcohol/PBS (1/40; Sigma-Aldrich), followed by subcutaneous injection of 25 ng IgE in 25 μl PBS in the right ear and 25 μl PBS in the left ear. 24 h later, mice were anesthetized and 200 μl antigen (100 μg DNP-HSA, 1% Evans blue in PBS) was injected intravenously via the retroorbital sinus. 30 min after the injection, mice were killed and both ears were removed. Ears were incubated in 200 μl formamide at 55°C for 48 h to extract the dye. Tissue debris was removed by centrifugation and the intensities of the dye were measured by absorption at 610 nm. The data are calculated as OD610 of the IgE-injected ear minus the OD610 of the PBS-injected ear from the same mouse.
Calcium flux.
BMMCs were sensitized with 1 μg/mL IgE for 4 h; resuspended at 107 cells/ml in Tyrode's buffer containing 3 μg/ml Indo-1 (Invitrogen) and 4 mM probencid; and incubated for 30 min at 37°C. Cells were washed twice with Tyrode's buffer and resuspended at 2 x 107 cells/ml. 40 μl of cells was added into 460 μl of prewarmed Tyrode's buffer to measure Ca2+ responses by flow cytometry (BD-LSR; Becton Dickinson). After collection of the baseline ratio of FL5 to FL4, 10 μl of 5 μg/ml DNP-HSA was added to stimulate cells. Calcium flux was assessed as the ratio of FL5 to FL4 fluorescence.
Online supplemental material.
For measurement of DGK transcript levels, RNA was isolated from WT and DGK–/– BMMCs by TRIzol extraction (Invitrogen) and cDNA generated by reverse transcriptions (CLONTECH Laboratories, Inc.). Transcripts were quantified by SYBR green real-time PCR using the following primers: DGK: 5'-GATGCAGGCACCCTGTACAAT-3', 5'-GGACCCATAAGCATAGGCATCT-3'; DGK: 5'-GGGACCTCAAGGACCTTGGT-3', 5'-TCAGCTCCTTGATCCCACAAA; and DGK: 5'-TTCCCCAGGGCACTCTCA-3', 5'-CAGACGTTGCATCTAGGAAGCA-3'. No products were amplified from a no reverse transcriptase control sample (unpublished data). Transcripts were normalized to GAPDH signal (5'-GAAGGTACGGAGTCAACGGATTT-3', 5'-GAATTTGACCATGGGTGGAAT-3') using the Ct method. For measurement of total cellular protein levels of PKC?II and PKC, WT and DGK–/– BMMCs were left unstimulated for 4 h in cytokine-free media with or without IgE (1 μg/ml). Cells were lysed in 1% NP-40 lysis buffer with protease inhibitors, proteins were resolved by SDS-PAGE, and Western blots were probed with antibodies to PKC?II or PKC. Blots were stripped and reprobed for actin as a loading control. Online supplemental material is available at http://www.jem.org/cgi/content/full/jem.20052424/DC1.
Acknowledgments
We thank J. Stadanlick for help in preparation of the manuscript; M. Jordan for help in the Ca++ experiment; S. Prescott and M. Topham for providing the anti-DGK antibody; E. Myers and E. Hainey for technical assistance; and Drs. Q.-C. Yu, H.-W. Yu, and Y. Wang for assistance in histological analysis.
This work was supported by the National Institutes of Health (G.A. Koretzky and X.-P. Zhong), from the Sandler Program for Asthma Research (G.A. Koretzky), and from the National Cancer Institute (B.A. Olenchock).
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