Integrin-mediated leukocyte adhesion is a critical aspect of leukocyte function that is tightly regulated by diverse stimuli, including chemokines, antigen receptors, and adhesion receptors. How cellular signals from CD31 and other adhesion amplifiers are integrated with those from classical mitogenic stimuli to regulate leukocyte function remains poorly understood. Here, we show that the cytoplasmic tail of CD31, an important integrin adhesion amplifier, propagates signals that induce T cell adhesion via β1 (VLA-4) and β2 (LFA-1) integrins. We identify the small GTPase, Rap1, as a critical mediator of this effect. Importantly, CD31 selectively activated the small Ras-related GTPase, Rap1, but not Ras, R-Ras, or Rap2. An activated Rap1 mutant stimulated T lymphocyte adhesion to intercellular adhesion molecule (ICAM) and vascular cell adhesion molecule (VCAM), as did the Rap1 guanine nucleotide exchange factor C3G and a catalytically inactive mutant of RapGAP. Conversely, negative regulators of Rap1 signaling blocked CD31-dependent adhesion. These findings identify a novel important role for Rap1 in regulating ligand-induced cell adhesion and suggest that Rap1 may play a more general role in coordinating adhesion-dependent signals during leukocyte migration and extravasation. Our findings also suggest an alternative mechanism, distinct from interference with Ras-proximal signaling, by which Rap1 might mediate transformation reversion.
In addition to soluble mitogenic stimuli, a number of leukocyte cell surface molecules have been shown to regulate integrin-mediated leukocyte adhesion. One particular receptor, CD31, a platelet endothelial cell adhesion molecule (PECAM-1) (Newman 1997), stimulates integrin-dependent adhesion in a wide variety of vascular cells, including leukocytes and platelets, via a process termed adhesion amplification (Tanaka et al. 1992; Berman and Muller 1995; Berman et al. 1996; Ranger et al. 1997). Numerous studies have also demonstrated a critical role for CD31 in mediating integrin-dependent leukocyte chemotaxis and extravasation in vitro and in vivo (Berman et al. 1996; Newman 1997; Duncan et al. 1999). The molecular basis for this has remained obscure, but recent studies have demonstrated that, in addition to mediating homophilic cell adhesion (Newton et al. 1997), CD31 acts as an adhesion-dependent signaling receptor (Newman 1997; Newton et al. 1997; Pumphrey et al. 1999). CD31 ligation stimulates tyrosine phosphorylation of CD31, leading to its association with a number of cytoplasmic signaling proteins, including SHP-1, SHP-2, SHIP, and PLC-γ1, suggesting that CD31 functions as a dynamic modulator of vascular cell behavior (Newman 1997; Newton et al. 1997; Pumphrey et al. 1999).
Several reports suggest a role for Ras family GTPases in the control of integrin-mediated adhesion. Ras superfamily GTPases cycle between inactive GDP-bound forms and active GTP-bound forms, and exchange for GTP and hydrolysis of GTP to GDP are catalyzed by guanine nucleotide exchange factors (GEFs) and GTPase activating proteins (GAPs), respectively (Bos 1997, Bos 1998). Use of active and dominant-negative mutants of H-Ras and R-Ras has revealed that these enzymes can regulate coupling of β1 and β2 integrin-dependent adhesion to T cell receptor (TCR/CD3), interleukin-3, and chemokine receptor signaling in T lymphocytes and pro-B cell leukemic cell lines (Zhang et al. 1996; O'Rourke et al. 1998; Liu et al. 1999; Shibayama et al. 1999; Tanaka et al. 1999). We have examined whether CD31 stimulates integrin-dependent adhesion via an intracellular signaling pathway, and if so, whether members of the Ras family were involved in this process. We find that the cytoplasmic tail of CD31 is essential for CD31-induced adhesion, and that Rap1 is specifically and selectively involved in this process.
Materials and Methods
Hemagglutinin (HA)-tagged Rap1 (Rap), RapV12, and H-RasV12 in the mammalian expression vector pMT2HA, pRSV, and pRSV-RapN17 have been described previously (Zwartkruis et al. 1998). pMT2HA-R-RasV38 was generated by subcloning a full-length NcoI (Klenow-filled)/XhoI fragment of R-RasV38 into NotI (mung bean nuclease-digested)/XhoI-digested pMT2HA. A SalI/NotI fragment encoding amino acids 200–297 of human RalGDS was amplified by PCR to generate pMT2HA-RalGDS-RBD. pMT2-HA-RapGAP was generated by subcloning full-length RapGAP (provided by Dr. Paul Polakis, Onyx Pharmaceuticals, Richmond, CA) as a SalI/BglII fragment into pMT2HA. Catalytically inactive RapGAP LIG was generated by mutating RapGAP amino acids 284–286 (RKR) to LIG using the Stratagene Quick site-directed mutagenesis kit. All PCR-generated sequences were checked by DNA sequencing. pCAGGS-C3G and pSR-His-tagged Spa1 were provided by Drs. Michiyuki Matsuda (National Institutes of Health, Tokyo, Japan) and Masakazu Hattori (Kyoto University, Kyoto, Japan), respectively.
Jurkat T cell lines were maintained as described previously (Reedquist and Bos 1998). The Jurkat cell line JHM1 2.2 was provided by Dr. Doreen Cantrell (Imperial Cancer Research Fund, London, UK), with kind permission of Dr. Art Weiss (University of California at San Francisco, San Francisco, CA). Jurkat cells used to generate CD31 wild-type (WT), CD31 glycosylphosphatidylinositol (GPI), and Y663/686F stable transfectants were provided by Dr. D. Samson (University of Bath, Bath, UK). CD31+ and CD31− variants were established by six rounds of MACs-sorting of parental Jurkat cells with anti-CD31 antibody 10B9. The negative variant was transfected with CD31 WT, CD31 GPI, or CD31 Y663/686F cDNA in pCDNA3 (Jackson et al. 1997; Newton et al. 1997), and stable polyclonal lines established by selection in G418 (1 mg/ml) and FACS sorting. Jurkat cells were transiently transfected by electroporation with 35 μg plasmid DNA. Jurkat cells (1.2 × 107 cells/ml in 0.4 ml complete media) were pulsed at 250 V and 960 μF with 5 μg TK-luciferase plasmid DNA, construct plasmids as indicated in figure legends, and added vector plasmid to keep DNA amounts constant. 24 h after transfection, cells were transferred to serum-free media and used 42–48 h after transfection for adhesion assays. Subconfluent A14 and COS-7 cells were transfected by calcium phosphate precipitation as described previously (Zwartkruis et al. 1998).
Anti-CD3 antibody T3b was kindly provided by Dr. Hergen Spits (Netherlands Cancer Institute, Amsterdam, The Netherlands). Antiintegrin β2 antibody L15, activating antiintegrin β1 antibody TS2/16, and activating antiintegrin β2 KIM185 have been described previously (van de Wiel-van Kemenade et al. 1992; Andrew et al. 1993). mAb 24, recognizing a ligand-induced epitope of αL, was kindly provided by Dr. Nancy Hogg (Imperial Cancer Research Fund, London, UK). Anti-CD31 antibodies, PECAM 1.2 and PECAM 1.3, were generous gifts from Dr. Peter Newman (Blood Center of Southeastern Wisconsin, Milwaukee, WS). Anti-CD31 antibodies 2H8, WM59, GI18, and 9G11 have been described previously (Yan et al. 1995; Newton et al. 1997). Other mAbs used in these studies were anti-Rap1, RalA, and Ras antibodies (Transduction Laboratories). Rabbit polyclonal anti-Rap2 and R-Ras antibodies were from Santa Cruz.
Purification of GST-RBD fusion proteins and their use in detecting activated Rap1, Rap2, Ras, and R-Ras by precipitation, SDS-PAGE, and immunoblotting have been described previously (de Rooij and Bos 1997; Franke et al. 1997; Reedquist and Bos 1998). Detection of bound radiolabeled GDP and GTP to Rap1 was also described previously (Zwartkruis et al. 1998).
For adhesion assays, transiently transfected Jurkat cells were harvested, washed, and resuspended in TSM media (20 mM Tris, pH 8, 150 mM NaCl, 1 mM CaCl2, 2 mM MgCl2). 96-well Costar Maxisorp plates were coated overnight at 4°C with goat anti–human IgG antibodies (Jackson ImmunoResearch; 4 μg/ml in TSM), washed, blocked for 30 min at 37°C with 1% BSA/TSM, followed by incubation 1 h at 37°C with 50 ng/ml recombinant intercellular adhesion molecule (ICAM)-1 or vascular cell adhesion molecule (VCAM)-1 human IgG Fc fusion proteins. The 50-μl cell suspension was mixed with 50 μl TSM or TSM with stimuli indicated. Cells were allowed to adhere for 30–60 min, and nonadherent cells removed with warm 0.5% BSA/TSM. Adherent cells were lysed and subjected to luciferase assays as described previously (Medema et al. 1992). Expression of transfected constructs was confirmed by immunoblotting of total cell lysates. Cells bound were calculated and were corrected for transfection efficiency and nonspecific effects of constructs by measuring luciferase activity of total input cells. Comparison of effects of cDNA construct overexpression on adhesion were made by paired t test or unpaired t test as appropriate. Fluorescent labeling of stably transfected cells with 2'7'-bis-(2-carboxyethyl)-5-(and-6)-carboxy fluorescein acetoxymethyl ester (Molecular Probes) and measurement of adherent cells with a Fluoroscan Ascent fluorescent plate reader (Lab Systems) has been described previously (Newton et al. 1997).
Flow cytometric analysis of transfected cells was performed by cotransfecting Jurkat JHMI cells with 1 μg pCMV-EGFP C1 plasmid (Promega) and the indicated cDNA constructs. After overnight serum starvation, cells were equilibrated in 0.5% BSA/1 mM CaCl2/PBS (FACS buffer) and left unstimulated, or stimulated for 30 min with plate-immobilized anti-CD31 antibody 2H8 (10 μg/ml). Cells were harvested, resuspended in FACS buffer containing primary antibodies (10 μg/ml), and incubated for 30 min on ice, or 37°C for mAb 24 epitope expression. For mAb 24 staining, additional sets of transfected cells were coincubated with 400 μM MnCl2 during primary antibody staining. Cells were washed with FACS buffer and stained with secondary rabbit anti–mouse RPE-Cy5-conjugated antibodies (Dako). Fluorescence intensity of EGFP-transfected cells was determined using a FACs Caliber flow cytometer and CellQuest software (both from Becton Dickinson).
Results and Discussion
Previously, CD31 has been demonstrated to stimulate T lymphocyte adhesion to ICAM and VCAM via T cell LFA-1 (αLβ2 integrin) and VLA-4 (α4β1 integrin), respectively (Tanaka et al. 1992). To examine whether CD31-stimulated integrin-dependent adhesion in T cells was regulated by signals generated through the CD31 cytoplasmic tail or via interactions using the extracellular domain of CD31 (Hemler 1998), we made use of Jurkat cells stably expressing full-length CD31 (CD31 WT), a GPI-anchored CD31 construct, previously shown to mediate CD31 homophilic binding (Newton et al. 1997), but lacking the CD31 cytoplasmic tail, or full-length CD31 containing two tyrosine-to-phenylalanine mutations (Y663/686F) in the major tyrosine-phosphorylation sites of the CD31 cytoplasmic tail (Pumphrey et al. 1999). CD31 expression of parental, CD31+- and CD31−-selected variants, and stable transfectants is shown in Fig. 1 A, and was equivalent in CD31 WT, CD31 GPI, and Y663/686F lines. All cell lines also expressed similar levels of αL, α4, α5, β1, and β2 integrins (data not shown). Although all cell lines adhered to ICAM-1 and VCAM-1 when stimulated by PMA (data not shown), only CD31 WT transfectants, but not CD31 GPI and Y663/686F cells, adhered to ICAM-1 or VCAM-1 after stimulation with anti-CD31 antibodies (Fig. 1 B). This suggested that CD31-induced, integrin-mediated adhesion requires intracellular signaling pathways generated by the cytoplasmic tail of CD31, specifically tyrosine phosphorylation of tyrosine residues 663 and/or 686, but not signaling pathways mediated by cis-interactions of the CD31 extracellular or transmembrane domains.
To address which Ras family members, if any, might participate in CD31 signaling, we precipitated endogenous GTPases from lysates of CD31-stimulated Jurkat cells with GST fusion proteins of Ras family-binding domains (RBDs) of Raf and RalGDS, which bind with high selectivity and specificty to activated Ras and Rap GTPases, respectively (de Rooij and Bos 1997; Franke et al. 1997). Immunoblotting of precipitated GTPases provides a qualitative representation of GTPase activation status after cell stimulation, corresponding to quantitative changes detected using classical GDP/GTP-binding ratio techniques. Time course analyses of Jurkat cells treated with anti-CD31 antibodies or TPA (Fig. 2 A) surprisingly revealed a rapid activation of the Ras-related GTPase, Rap1, by CD31, which was maximal 2–5 min after stimulation and decreased slowly toward basal levels after 20 min. In contrast, whereas both Rap1 and Ras were activated by TPA, CD31-dependent stimulation of Rap1 was highly selective and no activation of Rap2, Ras, or R-Ras was noted at any point during this time course. Both Rap1 and Ras, but not the other GTPases tested, were also activated by TCR stimulation (data not shown). GTP-bound R-Ras was detected in Raf-RBD pull-downs only after longer exposures of films, reflecting the relatively low levels of R-Ras protein expression in Jurkat cells. R-Ras protein expression was at least tenfold lower in Jurkat cells as compared with A431 fibroblasts, while Rap1, Rap2, and Ras levels were relatively equivalent (Fig. 2 A, right, last two lanes).
Functional anti-CD31 antibodies against CD31 extracellular domains 1 and 6 (PECAM 1.2, PECAM 1.3, and 2H8), activated Rap1 more potently than nonfunctional antibodies (WM59, 9G11, and GI18; Fig. 2 B), correlating with the ability of these antibodies to induce CD31-dependent adhesion (Newton et al. 1997). Additionally, activation of Rap1 by anti-CD31 antibodies was observed in CD31 WT Jurkat cell transfectants, but not CD31 GPI or Y663/686F transfectants (Fig. 2 C), demonstrating a correlative requirement for the CD31 cytoplasmic tail in the activation of Rap1 and induction of adhesion.
As CD31 stimulation selectively activated Rap1, and Rap1 activation correlated with CD31-dependent adhesion to ICAM and VCAM, we next addressed whether constitutive activation of Rap1 was sufficient to induce adhesion. Jurkat T cells transiently transfected with a luciferase reporter plasmid and indicated cDNA constructs were allowed to bind to immobilized recombinant ICAM and adhering transfected cells detected by measurement of luciferase activity. T cells expressing constitutively active Rap1 (RapV12) or the Rap1 GEF C3G (Tanaka et al. 1994) displayed ∼3.5- and 3-fold increases in adhesion to ICAM, respectively (Fig. 3 A). C3G-induced spreading and adhesion on fibronectin has been observed previously in 32-D cells, although involvement of Rap1 was not examined and Ras, R-Ras, or other GTPases were implicated (Arai et al. 1999). Expression of either the active form of Ras (RasV12) or R-Ras (R-RasV38) resulted in a lower, but detectable induction of adhesion (1.5–2-fold). However, RasV12-stimulated adhesion was not statistically significant, RasV12 stimulated adhesion in only two of five experiments, and RapV12-induced adhesion was always higher than that induced by RasV12 and R-RasV38, even though the latter two constructs were expressed at significantly higher levels than RapV12 (Fig. 3 A, left inset). Introduction of a RapGAP mutant (RapGAP-LIG; Rubinfeld et al. 1991), containing a substitution of amino acids 284–286 in the RapGAP arginine finger critical for RapGAP catalytic activity (RKR, mutated to LIG), which, unlike wild-type RapGAP, displays no GAP activity toward Rap1 (Fig. 3 B), increased the number of ICAM-bound cells to a similar level as observed with RapV12 and C3G. RapGAP-LIG may perturb Rap1 signaling by displacing endogenous RapGAP from a subcellular localization required for downregulating Rap1 or may constitutively associate with basally activated Rap1 and serve as an effector protein linking Rap1 to an as yet unidentified target.
We next examined if inhibition of Rap1 signaling would abolish CD31-dependent adhesion to ICAM. Therefore, we introduced a putative dominant-negative mutant of Rap1, RapN17, into cells. RapN17 did not affect basal adhesion of Jurkat cells to ICAM, but completely abolished CD31-dependent increases in adhesion (Fig. 3 C). Although the RapN17 mutation was modeled on the corresponding dominant-negative mutation in H-Ras (Medema et al. 1991), RapN17 is not considered to function as a strict dominant-negative protein. Whereas RasN17 blocks Ras signaling by sequestering Ras GEFs, RapN17 fails to bind to Rap1 GEFs in vitro (van den Berghe et al. 1997), and fails to inhibit EGF-dependent activation of cotransfected wild-type Rap1 in COS-7 cells (Wolthuis, R.M.F., and J.L. Bos, unpublished observation).
Because of uncertainties in the mechanism by which RapN17 might block CD31-stimulated adhesion, we sought independent confirmation that Rap1 was required for CD31-induced adhesion of Jurkat cells to ICAM. Transient expression of the Rap1-specific GAP, RapGAP, resulted in a strong reduction of basal adhesion to ICAM, and significantly reduced CD31-dependent adhesion (Fig. 3 C). This result is compatible with the notion that a Rap1GAP should decrease levels of GTP-bound Rap1 (see Fig. 3 B), but should still allow ligand-induced activation of Rap1. Finally, we used the Rap1 binding domain of RalGDS, RBD, which binds with high affinity and specificity to GTP-bound Rap1 in vitro (Franke et al. 1997). This fragment is hypothesized to block effector binding to Rap1. Expression of RBD significantly abolished both basal and CD31-induced adhesion to ICAM (Fig. 3 C). Thus, using three independent strategies for interfering with Rap1 signaling, overexpression of inactive Rap1, Rap1-specific RapGAPs, and an isolated RBD of a Rap-binding protein, these experiments demonstrate a critical role for Rap1 in mediating CD31-induced adhesion to ICAM.
To address whether Rap1 selectively regulated β2 integrins (LFA-1) on Jurkat cells, or if it was also coupled to the regulation of β1 integrins (VLA-4), we examined the effects of activating and inactivating mutants of Rap signaling on Jurkat cell adhesion to VCAM. Stimulation of CD31 resulted in a smaller induction of adhesion to VCAM (1.5–2-fold increase; Fig. 4 A) than observed to ICAM, in part due to the higher basal level of adhesion observed on VCAM (typically 30–50%, compared with 10–20% on ICAM). A similar increase was also observed in cells expressing RapV12, C3G, and mutant RapGAP-LIG, but not RasV12 or R-RasV38. Conversely, RapN17, RapGAP, and a second GAP for Rap1, Spa1 (Kurachi et al. 1997), significantly reduced basal Jurkat cell adhesion to VCAM, and strongly blocked CD31-dependent adhesion (Fig. 4 B).
It has been reported previously that Ras regulates TCR-stimulated lymphocyte adhesion to ICAM (O'Rourke et al. 1998; Tanaka et al. 1999). As we failed to detect Ras activation by CD31, and RasV12 did not induce a clear increase in adhesion to ICAM or VCAM, it is unlikely that Ras mediates the main signaling pathway from CD31 stimulation to integrin-mediated adhesion. However, overexpression of RasN17 did inhibit CD31-dependent adhesion to VCAM (data not shown), suggesting that Ras might also contribute to adhesion responses.
Integrin-dependent adhesion can be regulated by changes in integrin surface expression, integrin surface distribution (avidity), or induction of conformational changes that increase integrin ligand affinity (Stewart and Hogg 1996). To investigate at which level Rap1 might influence cell adhesion, we first examined if Rap signaling affected LFA-1 expression levels. Jurkat cells were cotransfected with EGFP as a reporter marker, along with indicated Rap1 signaling pathway cDNA constructs. Staining of transfected cells with anti-β2 integrin antibody revealed that overexpression of RapV12, RapN17, RBD, RapGAP, or RapGAP LIG failed to influence surface expression levels of LFA-1 (Fig. 5 A). CD31 expression levels were also unaffected (data not shown). Similarly, RapV12, RapGAP LIG, RapGAP, and RapN17 failed to induce LFA-1 surface clustering, as detected with the NKI-L16 antibody (data not shown), although active RasV12 induced clustering of LFA-1, as previously reported (Tanaka et al. 1999).
The anti-αL integrin antibody mAb 24 recognizes a conformation-dependent ligand-induced epitope on LFA-1, and induction of the mAb 24 epitope correlates with increased LFA-1 affinity for ICAM (Dransfield and Hogg 1989). TCR and TPA-induced mAb 24 epitope expression previously have been found to be dependent on the presence of ICAM, suggesting that signals generated by TCR and TPA facilitate weak basal interactions between LFA-1 and ICAM, stabilizing LFA-1 in a high-affinity conformation (Cabanas and Hogg 1993). This conformational change can also be induced by LFA-1 exposure to Mn2+, independently of “inside-out” signaling. We found that anti-CD31 stimulation of Jurkat cells, or Jurkat cells transfected with GFP alone, resulted in an ∼1.5-fold increase in mAb 24 expression (Fig. 5 B and data not shown), whereas a 2.25–2.5-fold increase was observed in Mn2+-treated cells. Incubation of cells with mAb 24 at 4°C abolished CD31 and Mn2+-induced mAb 24 expression to background levels (data not shown), consistent with the temperature sensitivity of the mAb 24 epitope (Dransfield and Hogg 1989). Although RapV12 expression had no statistically significant effect on basal or induced mAb 24 epitope expression, RapN17 and RBD abolished induction of the mAb 24 epitope by CD31 and Mn2+. Conversely, RapGAP LIG enhanced CD31- and Mn2+-induced expression of the mAb 24 epitope. RapN17 also inhibited the increase in the percentage of mAb 24-reactive cells observed after CD31 or Mn2+ treatment (Fig. 5 C). Thus, our studies suggest that whereas Rap does not directly stimulate activation of LFA-1, signaling via Rap1, or basal activation of Rap1, appears to be a requisite factor for stabilization of the active conformation of LFA-1. Moreover, our finding that RapN17 blocks direct conformational changes induced by extracellular Mn2+ may suggest that inactive Rap may act to lock LFA-1 in an inactive conformation. Consistent with this model, overexpression of RapN17, RapGAP, or RalGDS RBD significantly blocked Mn2+-induced adhesion of Jurkat cells to immobilized ICAM, whereas RapV12 augmented the induced cell adhesion (Fig. 5 D).
Our report is the first example of requisite involvement of Rap1 in coupling cell surface receptor stimulation to integrin-mediated adhesion. Previously, it was shown that Rap1 is activated after stimulation of a large variety of cell surface receptors, including B and T cell antigen receptors, chemokine and cytokine receptors (including fMLP, PAF, and GM-CSF), and receptors for platelet agonists (thrombin, thromboxane A2, and ADP; reviewed in Bos 1997). Many of these receptors have been implicated in the control of integrin-mediated adhesion. Furthermore, the involvement of Rap1 in the control of cell adhesion recently has been suggested by studies in which Spa1 was found to inhibit G-CSF–induced adhesion of 32-D cells to culture dishes (Tsukamoto et al. 1999). Also, FcεRI-mediated adhesion of RBL cells to culture dishes is inhibited by expression of RapGAP (M'Rabet 1999). Therefore, it is plausible to propose that one of the functions of Rap1 is to control integrin-mediated adhesion.
The mechanism by which Rap1 signaling modulates integrin function is unknown, although our data suggest that Rap1 may regulate the ability of LFA-1 to undergo ligand-induced conformational changes. This effect could be direct, by binding of Rap1 to integrins or integrin-associated complexes. Interestingly, Rap2, a very close relative of Rap1, has been found in complex with the αIIbβ3 integrin (Torti et al. 1999), although no extracellular stimuli coupling to Rap2 activation have been identified. Alternatively, Rap1 may stimulate effector pathways that regulate integrins. Putative downstream signaling pathways of Rap1 include B-Raf/MAP kinase cascade and Ral GTPase GEFs (Bos 1997, Bos 1998), although we have not detected CD31-dependent activation of MAP kinase or Ral in Jurkat cells (data not shown). Novel binding partners of activated Rap1 recently identified in vitro, Krit1 (Serebriiskii et al. 1997) and AF6 (Linnemann et al. 1999), are proteins lacking any obvious enzymatic activity and are thought to associate with cytoskeletal components. Our identification of integrin-adhesion as a physiological target of Rap1 should facilitate identification of Rap1 effectors. Finally, the unique coupling of CD31, which is also expressed on vascular cells, to Rap1 suggests a critical role for Rap1 in mediating not only leukocyte adhesion, but other integrin-dependent events mediated by CD31 that require platelet and leukocyte interactions with vascular endothelial cells, including leukocyte transmigration and extravasation. Interestingly, regulation of integrin adhesion might also explain the flat revertant phenotype of Ras-transformed cells expressing Rap1 (Kitayama et al. 1989).
We thank Drs. Peter Newman for the generous gifts of PECAM 1.2 and 1.3 antibodies and CD31 cDNA constructs, Nancy Hogg (Imperial Cancer Research Fund, London) for mAb 24 antibody, Doreen Cantrell (Imperial Cancer Research Fund, London) for Jurkat JHMI cells, and Hergen Spits (The Netherlands Cancer Institute, Amsterdam) for anti-CD3 T3b antibody. We are grateful to Veronique Smits and Dr. Rene Medema (Utrecht University) for assistance with FACS analysis, and Miranda van Triest (our laboratory) for excellent technical assistance.
K.A. Reedquist was supported by a postdoctoral fellowship from the Netherlands Royal Academy of Sciences (KNAW). F.J.T. Zwartkruis and R.M.F. Wolthuis were funded by the Dutch Cancer Society. E. Ross and C.D. Buckley were supported by grants from the Nuffield Foundation (RHE/97/273) and the Wellcome Trust, respectively.
Abbreviations used in this paper: GAP, GTPase activating protein; GEF, guanine nucleotide exchange factor; GPI, glycosylphosphatidylinositol; GST, glutathione-S-transferase; HA, hemagglutinin; ICAM, intercellular cell adhesion molecule; PECAM, platelet endothelial cell adhesion molecule; RBD, Ras-binding domain; VCAM, vascular cell adhesion molecule; WT, wild-type.