LFA-1–mediated Adhesion Is Regulated by Cytoskeletal Restraint and by a Ca²⁺-dependent Protease, Calpain

Ionomycin, thapsigargin, phorbol 12,13 dibutyrate (PdBu), and the membrane soluble calpain inhibitor calpeptin were obtained from Calbiochem/ Novabiochem Corp. (La Jolla, CA); dBHQ, and the calpain inhibitor, CBZ-LVG, were purchased from Sigma Chemical Co. (Dorset, UK). Jasplakinolide was obtained from Molecular Probes, Inc. (Eugene, OR). SK&F 96365 was purchased from BiomoL Feinchemikalien GmbH (Hamburg, Germany). With the exception of SK&F 96365, which was directly soluble in H₂O, stock concentrations of inhibitors were prepared in DMSO and in every relevant experiment an equivolume of DMSO was added in the control sample. The above reagents had no effect on the viability of the T cells at the levels used in the reported experiments.

A dimeric form of an ICAM-1Fc chimaeric protein consisting of the five extracellular domains of ICAM-1 fused to the Fc fragment of human IgG1 was prepared as previously described (Berendt et al., 1992). Flow cytometry and measurement of the binding of soluble recombinant ICAM-1Fc to T cells was carried out as previously described (Stewart et al., 1996). mAbs used in this study were the LFA-1 α subunit (CD11a) mAbs 38 (Dransfield and Hogg, 1989), F110.22 (Schmidt, 1989), and G25.2 (Becton and Dickinson Co., Mountain View, CA). The anti-CD3 mAbs G19.4 and UCHT1 were obtained from Bristol Myers Squibb (Seattle, WA) and P. Beverley (University College, London), respectively. The secondary FITC-conjugated antibodies goat anti–mouse IgG Fc and goat anti–human IgG Fc were obtained from Jackson ImmunoResearch Laboratories, Inc. (West Grove, CA).

T lymphoblastoid cells were expanded from unstimulated peripheral blood mononuclear cells by culture for 1–2 wk in RPMI-1640 medium containing recombinant IL-2 (20 ng/ml; Cetus Corp., Berkeley, CA) with details as previously described (Dransfield et al., 1992). Cells were used between days 10 and 14. The method for quantifying T cell adhesion to ICAM-1Fc protein has been previously described (Stewart et al., 1996), with the exception that the assay buffer used was RPMI 1640 unless controlled cation conditions were being analyzed. For these experiments T cells were treated with 5 mM Mg²⁺/1 mM EGTA in Hepes/NaCl buffer. The ICAM-1Fc protein was coated at 0.24 μg/well onto 96-well Immulon 1 plates (Dynatech, Chantilly, VA).

For immunofluorescence analysis by confocal microscopy, 13-mm-round glass coverslips were precoated with a 0.01% solution of poly-L-lysine (Sigma Chemical Co.) for 10 min at room temperature, washed twice in RPMI 1640, and then left to air dry. T cells were washed three times in RPMI 1640 buffer before addition onto coverslips (5 × 10⁵ cells/coverslip), in the presence of stimulants and CD11a mAbs at 10 μg/ml. Coverslips were spun at 40 g, and then incubated for 30 min at 37°C. Unbound cells were removed by gentle washing in warm RPMI 1640 buffer. To prevent antibody-induced clusters, cells were fixed with 1% formaldehyde in PBS-A for 10 min at room temperature before a second incubation with 10 μg/ml FITC-conjugated goat anti–mouse IgG Fc (Jackson ImmunoResearch Laboratories) for 25 min at 4°C. Cells stimulated via CD3 triggering were incubated with CD3 mAbs UCHT1 or G19.4 for 30 min at 37°C and fixed as above.

Cells were mounted for confocal microscopy which was carried out using a MRC-600 Confocal Laser Scanning System (Bio-Rad Laboratories Ltd, Hertfordshire, UK). The regions of the confocal microscopy images with the highest fluorescence intensity (i.e., with the pixel color intensity in the 150–255 range) were highlighted in red using the segmentation utility of the IP Lab Spectrum Version 3.1 software (Signal Analytics Co., Vienna, VA).

This software was also used to quantify the levels of fluorescence on the images. Background fluorescence was estimated by measuring the signal strength in areas visibly devoid of specific staining but in close proximity to cells. The average of these values was then subtracted from the original image to give a corrected image. The areas of interest (e.g., free membrane or membrane at cell–cell contact points) on the corrected images were selected and the average signal strength calculated automatically by the computer software. A statistical assessment of the differences between the treatment groups and the untreated resting T cells was performed using the one-way ANOVA test.

To gain insight into the role of Ca²⁺ in LFA-1 adhesion, we have analyzed the effect on leukocyte adhesion to ICAM-1 of the Ca²⁺ ionophore ionomycin and two other Ca²⁺ mobilizers, thapsigargin, and dBHQ. The latter two compounds act by inhibiting the ATPase pumps on Ca²⁺ storage organelles, which maintain homeostasis by pumping Ca²⁺ from the cytosol into these organelles and the endoplasmic reticulum (Thomas and Hanley, 1994). Inhibition of pump action causes emptying of intracellular Ca²⁺ stores and a resultant Ca²⁺ influx across the plasma membrane via capacitative entry (Thastrup et al., 1990). The three agents showed a dose-dependent stimulation of T cell LFA-1–mediated adhesion to immobilized ICAM-1 (Fig. 1). The peak adhesion with ionomycin, thapsigargin, and dBHQ occurred at 0.7, ∼5, and ∼50 μM, respectively. The higher optimal concentration of dBHQ may be due to its comparatively poor ability to penetrate the plasma membrane (Thomas and Hanley, 1994). The reason for the phase of decline in the bell-shaped response curves was not due to loss of cell viability, but was not further pursued. Therefore, mobilization of [Ca²⁺]_i by three distinct agents can cause LFA-1–mediated T cell adhesion, highlighting a role for [Ca²⁺]_i in the LFA-1 activation pathway.

The tested pharmacological agents raise [Ca²⁺]_i levels not only by inducing release from intracellular stores, but also by capacitative fluxing in through the plasma membrane (Putney and Bird, 1993; Breittmayer et al., 1994; Wenzel-Seifert et al., 1996). To define the source of Ca²⁺ that facilitates T cell adhesion, we made use of the imidazole compound SK&F 96365, which blocks Ca²⁺ channels on leukocytes that open as a result of depletion of Ca²⁺ stores (Wenzel-Seifert et al., 1996). Adhesion stimulated by ionomycin, thapsigargin, through the TCR–CD3 complex, and by PdBu was inhibited by SK&F 96365 (Fig. 2). As expected, T cell adhesion to ICAM-1 induced by Mg²⁺/EGTA was not altered by the Ca²⁺ channel blocker (Stewart et al., 1996). Further evidence that extracellular Ca²⁺ has an intracellular function came from the use of the intracellular Ca²⁺ chelator BAPTA–AM, which at 20–30 μM reduced LFA-1 adhesion by 50–80% for all inducers in this study with the exception of Mg²⁺/EGTA (data not shown). Therefore, adhesion stimulated in several ways by “inside out” signaling is dependent upon an extracellular source of Ca²⁺.

To investigate the mechanism of Ca²⁺ action, the characteristics of LFA-1–mediated adhesion caused by the Ca²⁺ mobilizers was examined. One question of interest was whether the Ca²⁺-mediated signaling increased the ability of LFA-1 to bind soluble ICAM-1 (sICAM-1). In a previous study, sICAM-1 binding distinguished high affinity Mg²⁺-stimulated LFA-1 from low affinity LFA-1 on phorbol ester-stimulated and XL-TCR–CD3 T cells (Stewart et al., 1996). None of the Ca²⁺ mobilizers showed any induction of sICAM-1 binding even at sICAM-1 levels of 1 mg/ml (4.5 μM), in contrast to the enhanced ability of Mg²⁺-stimulated T cells to bind sICAM-1, which served as a positive control (Fig. 3). It can be concluded that the Ca²⁺ mobilizers resemble the phorbol ester or TCR–CD3 model of adhesion by failing to promote an increase in the ability of LFA-1 to bind to soluble ICAM-1.

As the Ca²⁺ mobilizers did not cause a detectable increase in the affinity of LFA-1, we used confocal microscopy to investigate whether the membrane distribution of LFA-1 was altered in a manner facilitating adhesion. To analyze LFA-1 distribution, we highlighted the confocal microscopy images such that the membrane regions with the highest LFA-1 fluorescence (i.e., in the pixel intensity range 150–250, where 250 is the highest possible value) are depicted in red and all others in white (Fig. 4). Unstimulated cells (Fig. 4,a) and Mg²⁺/EGTA–stimulated cells (Fig. 4,b) have very little high intensity LFA-1 fluorescence (red) in comparison to that of thapsigargin-stimulated cells (Fig. 4,c). These observations were confirmed by quantifying (see Materials and Methods) the levels of fluorescence for each sample on regions of the membrane where there was no contact between cells (Table I, Free membrane). Statistical analysis (one way ANOVA) of these measurements confirmed that the level of fluorescence on the thapsigargin-stimulated cells, but not on the Mg²⁺/EGTA–stimulated T cells, was significantly increased compared to the level on the resting T cells (Table I, Significance levels). This increase in the intensity of LFA-1 fluorescence upon thapsigargin stimulation was detected with three distinct CD11a mAbs, 38, F110.22, and G25.2 (data not shown), and therefore does not represent the exposure of a particular epitope. These results suggested that thapsigargin might stimulate an increase in the cell surface expression of LFA-1. When measured by flow cytometry, however, results revealed that the level of LFA-1 expression after thapsigargin stimulation did not differ from LFA-1 expression on the resting or Mg²⁺/EGTA–treated cells (Table I, Flow cytometry). This suggested that the increase in signal strength observed by confocal microscopy upon thapsigargin stimulation reflects increased clustering that creates a higher LFA-1 fluorescence intensity. Similar results were obtained with the other Ca²⁺-mobilizing agents, with PdBu, and by XL-TCR–CD3 (data not shown).

It was observed that some of the brightest LFA-1 fluorescence was found where cells were in contact with each other, and we therefore quantified the level of fluorescence in these regions (Table I, Contact zone) to determine whether this high fluorescence reflected a redistribution of LFA-1 to cell–cell contacts or was merely the additive value of the two cell membrane measurements. As the ratio of the average fluorescence intensity at cell contact areas to that of free membrane was ∼2 (Table I, Contact/Free), we concluded that there is no large scale redistribution of LFA-1 to points of cell contact upon thapsigargin treatment. In summary, the confocal results revealed that upon thapsigargin stimulation LFA-1 becomes clustered but does not change its distribution to regions of the cell membrane in contact with other cells. Similar results were obtained with the other Ca²⁺-mobilizing agents as well as PdBu (data not shown), and by cross-linking the TCR/CD3 (see Fig. 7) suggesting that local LFA-1 clustering may be a general feature of several T cell adhesion- activating protocols.

The implication of the above confocal experiments was that the Ca²⁺ mobilizers promoted LFA-1 clustering. This clustering might occur as a result of breakdown of cytoskeletal tethering (Elemer and Edgington, 1994; Kucik et al., 1996; Lub et al., 1997) or, conversely, might follow from the formation of new cytoskeletal connections (Pardi et al., 1992). To address these alternative possibilities, we investigated the effects on LFA-1 adhesion and membrane distribution of jasplakinolide, a compound that stabilizes pre-existing actin filaments, promotes actin polymerization, and prevents actin depolymerization (Bubb et al., 1994). Jasplakinolide caused dose-dependent inhibition of LFA-1–mediated adhesion to ICAM-1 with complete inhibition between 1 to 2 μM (data not shown). Therefore, the general inhibitory effects of jasplakinolide on agonists that indirectly stimulate LFA-1–mediated adhesion is consistent with a requirement for disassembly of the actin cytoskeleton.

We next used confocal microscopy to ask whether jasplakinolide affected the distribution of LFA-1 after pretreatment of thapsigargin-stimulated T cells. As seen in Fig. 5, jasplakinolide diminished the fluorescence levels of LFA-1 detected by confocal microscopy (i.e., there is less fluorescence highlighted [red] in Fig. 5 b than in a). Identical levels of LFA-1 expression were detected by flow cytometry before and after jasplakinolide treatment (data not shown), indicating that the inhibitor interfered with LFA-1 clustering rather than causing receptor loss. Similar results were obtained after T cell stimulation with phorbol ester and through CD3–TCR (data not shown). Therefore, clustering of LFA-1 on the membrane is dependent on the disassembly of the actin fibers, suggesting that adhesion through LFA-1 clustering is promoted by active release from restraints imposed by the cytoskeleton.

In an attempt to understand the molecular mechanism by which Ca²⁺ induces LFA-1 clustering, we investigated the effect of inhibitors and mAbs specific for several major Ca²⁺-using enzymes that have a link with adhesion. After stimulation with ionomycin or thapsigargin, we failed to find a role for PKC, calcineurin, or calmodulin using the specific inhibitors Ro 31-8220 (1–5 μM), FK506 (0–7 ng/ml), and trifluoperazine (0.5–10 μM), respectively. Similarly, immunoprecipitation and blotting with specific antibodies failed to show an association of the 208-kD MLCK (Gallagher et al., 1995) or calreticulin (Coppolino et al., 1995) with stimulated LFA-1 (data not shown).

Another enzyme activated by Ca²⁺ is calpain, a multifunctional protease that is located in the cytosol (Sorimachi et al., 1994). We monitored LFA-1 adhesion stimulated by thapsigargin, PdBu, XL-TCR–CD3, and Mg²⁺/EGTA after preincubation with the membrane permeable calpain inhibitor, calpeptin (Tsujinaka et al., 1988; Kwak et al., 1993). This agent caused maximal inhibition of T cell adhesion at 100 μg/ml (280 μM) after stimulation by thapsigargin, PdBu, and XL-TCR–CD3, but had no effect on Mg²⁺-induced adhesion (Fig. 6). A further calpain inhibitor, CBZ-LVG, also blocked adhesion at similar concentrations (data not shown). There was no alteration in cell viability at concentrations at which these inhibitors were maximally active. We next found that the levels of clustered LFA-1 detected after treatment with thapsigargin (Fig. 7,a), XL-CD3 (Fig. 7,b), and PdBu (data not shown) were diminished by calpeptin treatment (i.e., there is less fluorescence highlighted [red] in Fig. 7,c than in a and in Fig. 7,d than in b) to levels similar to those on resting T cells (Table I, Free membrane).

The calpain inhibitors used in this study are not entirely specific for calpain but also inhibit lysosomal cathepsins and proteasome activity. To rule out the involvement of the proteasome, we investigated the effect of the highly specific proteasome inhibitor lactacystin on T cell adhesion to ICAM-1. Although antigen presentation was inhibited by 20 μM lactacystin (Correa, I., and J. Trowsdale, personal communication) T cell adhesion was unaffected by concentrations as high as 200 μM (data not shown). Furthermore, T cells lack lysosomal cathepsins that are also susceptible to the calpain inhibitors. In summary, these results indicate that a calpain-like enzyme is pivotal in causing the clustering of LFA-1 and by this means adhesion to ICAM-1 is facilitated.

In this study, we have examined a role for Ca²⁺ in the induction of integrin-mediated adhesion, using the leukocyte integrin LFA-1 on T cells as the model. Three agents that cause Ca²⁺ mobilization trigger LFA-1–mediated adhesion to ICAM-1 to the same extent as other inside out inducers of adhesion such as XL-TCR–CD3 and phorbol ester. Furthermore, all three forms of stimulation cause LFA-1 clustering on T cells. The following points can be made about the Ca²⁺-dependent mechanism by which adhesion is brought about: (a) LFA-1 clusters in the cell membrane thereby strengthen adhesion by increasing the integrin avidity; (b) the adhesion is dependent upon Ca²⁺ influx; (c) the overall affinity of LFA-1 for ligand does not alter as no increase in the ability to bind soluble ICAM-1 can be detected; (d) both adhesion and LFA-1 redistribution are prevented by inhibiting cytoskeletal disassembly, implying a role for actin reorganization; (e) calpain has a central role in the clustering of LFA-1; (f) the above features are not shared by Mg²⁺/EGTA–treated LFA-1, which binds ICAM-1 with high affinity and mediates adhesion without dependence on the intracellular events described here.

Stimulation of T cells by the Ca²⁺ mobilizers, through the TCR–CD3 complex and by phorbol ester, results in an increase in integrin avidity by clustering of LFA-1 in the membrane. These results are in agreement with previous reports of integrin clustering after phorbol ester stimulation (Burn et al., 1988; Kupfer and Singer, 1989). Both phorbol esters and the other Ca²⁺-dependent adhesion inducers used in this study cause LFA-1 clustering over the entire cell membrane. In a more physiological setting, when the TCR is triggered upon T cell–APC contact Ca²⁺ fluxes occur locally (Zweifach and Lewis, 1993; Hall et al., 1993; Donnadieu et al., 1994; Negulescu et al., 1996). The subsequent effect on LFA-1 would be confined to the immediate points of cell contact. Support for this prediction comes from the observation that LFA-1 segregates away from the “TCR clusters” after TCR signaling, and therefore is no longer uniformly distributed (Dustin et al., 1996). Whether clustering involves direct lateral association between integrin subunits or is driven by ligand (Singer, 1992) requires further investigation. The expression of the epitopes of both nonfunction blocking (G25.2) and function blocking (38, F110.22) anti–LFA-1 α-subunit mAb epitopes is comparable when detected by confocal microscopy, implying that the clustering in this study is probably not driven by ligand (data not shown). The work of van Kooyk et al. (1994) suggests that Ca²⁺ may also have an extracellular role in integrin multimerization. Finally, a recent analysis of α4 integrin made use of the confocal microscope to investigate integrin clustering in the absence of an alteration in α4 integrin cell membrane expression (Yauch et al., 1997) in a similar manner to the approach described in our study.

Calpain is implicated in the clustering and adhesive activity of LFA-1 by the ability of selective inhibitors to diminish these processes. Calpains are Ca²⁺-dependent neutral cysteine proteases that are activated by local Ca²⁺ fluxes and are widely expressed in mammalian cells (Suzuki et al., 1987; Saido et al., 1994; Sorimachi et al., 1994). Calpain is highly expressed in T cells and is increased at both mRNA and protein levels by phorbol ester, calcium ionophore, and anti-CD3 treatment, all agents that can induce LFA-1 adhesion (Deshpande et al., 1995). In platelets Ca²⁺ ionophore will directly activate calpain, but when platelets are stimulated by a physiological agonist, such as thrombin, calpain activation is then dependent upon interaction of integrin αIIbβ3 with ligand (Fox et al., 1993). However, for T cells, the evidence suggests that the Ca²⁺ flux is not dependent on ligand binding by LFA-1, but, as we argue here, is directly responsible for LFA-1 clustering, with ligand binding a secondary event. Firstly, anti-CD3 stimulation of T cells causes activation of calpain proteolytic activity (Selliah et al., 1996). Secondly, the Ca²⁺ flux in T cells stimulated in this manner is not affected by function blocking CD11a and CD18 mAbs (Monard, 1991). Finally, there has been no indication that LFA-1 is physically associated with Ca²⁺ channel activity as has been suggested for αIIbβ3 (Rybak et al., 1988; Fujimoto et al., 1991). Therefore, the evidence suggests that calpain activity is regulated differently in these two cell types, but this does not preclude further action of calpain after the ICAM-1 binding phase of T cells.

There are a number of possibilities to explain how calpain might be acting. Calpain may be activated to cleave a key protein, physically releasing LFA-1 from its cytoskeletal restraint and allowing movement in the membrane as observed by single particle tracking (Kucik et al., 1996) and resonance energy transfer studies (Poo et al., 1994). Proteins that have been identified as calpain targets include talin (Inomata et al., 1996), filamin (Collier and Wang, 1982), and α-actinin (Selliah et al., 1996). In resting PBMC, both filamin and α-actinin are associated with CD18 (Pavalko and LaRoche, 1993; Sharma et al., 1995), and in T cells calpain cleaves α-actinin after TCR–CD3 triggering (Selliah et al., 1996) with kinetics similar to that of LFA-1–mediated adhesion (Dransfield et al., 1992; Dustin and Springer, 1989). Another possibility is that calpain cleaves a signaling protein. Potential candidates include focal adhesion kinase (Cooray et al., 1996) and phosphotyrosine phosphatase kinase 1B (Frangioni et al., 1993). It will be of interest to test the sensitivity to calpain of LFA-1–binding proteins such as cytohesin-1 (Kolanus et al., 1996). There is evidence that calpain can cleave the β3 subunit (Du et al., 1995). Whether the β2 subunit can also be cleaved by calpain remains to be investigated, and it is uncertain whether a β2 integrin cleaved at the sites homologous to the β3 calpain sensitive sites would be able to attach to the cytoskeleton or to bind ligand.

The cytoskeleton is intimately involved in the adhesive process. Use of jasplakinolide, an agent that inhibits actin disassembly (Bubb et al., 1994) prevents LFA-1 clustering and T cell adhesion. Alternatively, low levels of cytochalasin D promote integrin-mediated adhesion (Elemer and Edgington, 1994; Kucik et al., 1996; Lub et al., 1997; Yauch et al., 1997) and allow movement of the integrin in the membrane (Kucik et al., 1996). Put together, these findings indicate that in the nonactive state, LFA-1 is tethered to the cytoskeleton and release from this constraint allows motility leading to LFA-1 clustering and adhesion to ICAM-1. LFA-1 has also been reported to associate with cytoskeletal elements after activation (Pardi et al., 1992), and it is possible that clustered integrin, either before or after contact with ligand, might renew interaction with the cytoskeleton. The role of calpain in cytoskeletal rearrangements remains unresolved. Cytoskeletal reorganization may be necessary for the exposure of the proteolytic target of calpain or, conversely, calpain activation may lead to alterations in the cytoskeleton itself. Phorbol ester and other stimulants also cause coincident PKC and calpain translocation to the membrane (Pontremoli et al., 1989; Hong et al., 1995). In platelets activating agonists are reported to cause calpain to move from a generalized distribution in cells to a peripheral location (Fox et al., 1993), and this could be brought about by cytoskeletal reorganization.

Here we have provided evidence that the protease calpain plays a role in the regulation of LFA-1 adhesion induced by Ca²⁺ flux. This process involves an increase in ligand-binding avidity of the T cell through clustering of LFA-1 but no detectable increase in LFA-1 affinity. In many aspects this route to LFA-1 adhesion differs from that of Mg²⁺/EGTA treatment, which requires neither Ca²⁺ nor calpain but activates from the “outside” causing an affinity increase in LFA-1, indicating direct integrin conformational change (Stewart et al., 1996). Thus, there are two alternative pathways to LFA-1–mediated adhesion with different mechanisms. Migrating cells need adhesive contacts that can be rapidly made and easily broken. We suggest here that such contacts may be regulated through proteolysis and cytoskeletal control. On the other hand, once a leukocyte has arrived at an inflammatory site, migration is halted and stable cell–cell contacts form, which may then allow the bi-directional signaling necessary for other aspects of T cell function (Shaw and Dustin, 1997). High affinity adhesion would be an efficient means of facilitating these interactions and therefore it is of interest that the Mg²⁺ concentration of wound fluids is in favorable balance with Ca²⁺ and considerably higher than in normal plasma (Grzesiak and Pierschbacher, 1995). There is also evidence that this higher affinity LFA-1 may succeed the primary low affinity interaction of LFA-1 as a result of conformational change brought about by contact with ligand (Cabañas and Hogg, 1993).

In summary, our findings show that the Ca²⁺-regulated activation of calpain causes the clustering of LFA-1, possibly by cleaving a key cytoskeletal component. In vivo this Ca²⁺-induced clustering would be speculated to be confined to local sites of receptor triggering. Recent studies have outlined the phases of contact between T cells with antigen-presenting cells and highlight the importance of local Ca²⁺ fluxes in converting the motile “scanning” T cell into an immobile cell, stably engaged with its partner (Donnadieu et al., 1994; Negulescu et al., 1996). Our observations lead to the prediction that any receptor trigger which stimulates a Ca²⁺ flux in T cells would induce LFA-1 adhesion. It will be interesting to discover whether this mechanism is unique to control of LFA-1 adhesion or part of the adhesion mechanism for integrins found on other cells.

We gratefully acknowledge the help of Imperial Cancer Research Fund colleagues Rainer Pepperkok, Peter Jordan, Alex Stokes, and Andrew Edwards (Digital Imaging Microscopy Department) and Henry Potts (Medical Statistics Group) for performing the statistical analysis. We thank K.K. Wang (Parke Davis, Ann Arbor, MI) for discussion about calpain and A. Koffer (University College of London, London) and G. Nash (University of Birmingham, Birmingham, UK) for discussion about jasplakinolide. We thank T. Plesner (University of Copenhagen, Copenhagen, Denmark) for LFA-1 mAb F110.22, F. Pavalko (Indiana School of Medicine, Indianapolis, IN) for sharing unpublished data and for the kind gift of embMLCK-specific mAb, S. Dedhar (Terry Fox Institute, Vancouver, British Columbia, Canada) for antisera specific for calreticulin, and N. Clipstone (Stanford, Palo Alto, CA) for FK506. We thank colleagues Matthew Robinson, Birgit Leitinger, Joanna Porter, and Rebecca Newton for their helpful comments about the manuscript.

This work was supported by the Imperial Cancer Research Fund.

 
• dBHQ

  2,5-di-t-butylhydroquinone

 
• ICAM-1

  intercellular adhesion molecule-1

 
• LFA-1

  lymphocyte function-associate antigen-1

 
• MLCK

  myosin light chain kinase

 
• Pdbu

  phorbol 12,13 dibutyrate

 
• PKC

  protein kinase C

 
• sICAM-1

  soluble intercellular adhesion molecule-1

 
• TCR

  T cell receptor