Inflammation and thrombosis occur together in many diseases. The leukocyte integrin Mac-1 (also known as integrin αMβ2, or CD11b/CD18) is crucial for leukocyte recruitment to the endothelium, and Mac-1 engagement of platelet GPIbα is required for injury responses in diverse disease models. However, the role of Mac-1 in thrombosis is undefined. Here we report that mice with Mac-1 deficiency (Mac-1−/−) or mutation of the Mac-1-binding site for GPIbα have delayed thrombosis after carotid artery and cremaster microvascular injury without affecting parameters of haemostasis. Adoptive wild-type leukocyte transfer rescues the thrombosis defect in Mac-1−/− mice, and Mac-1-dependent regulation of the transcription factor Foxp1 contributes to thrombosis as evidenced by delayed thrombosis in mice with monocyte-/macrophage-specific overexpression of Foxp1. Antibody and small-molecule targeting of Mac-1:GPIbα inhibits thrombosis. Our data identify a new pathway of thrombosis involving leukocyte Mac-1 and platelet GPIbα, and suggest that targeting this interaction has anti-thrombotic therapeutic potential with reduced bleeding risk.
Thrombotic cardiovascular diseases, including myocardial infarction and stroke, are the leading cause of death in developed countries1. Current anti-thrombotic drugs, including antiplatelet agents and anticoagulants, are associated with significant bleeding risk and increased mortality2,3,4. There is emerging experimental evidence distinguishing the molecular and cellular mechanisms of haemostasis and thrombosis5,6, thereby providing potential therapeutic targets with reduced bleeding risk. One such area of research focus is ligand–receptor interactions, including CD40L and its binding to platelet GPIIb/IIIa (ref. 7), Gas6 and its tyrosine kinase receptors (mer, tyro3 and axl)8, ephrins and their eph kinase receptors9, and myeloid-related protein-8/14 (MRP-8/14 or S100A8/A9) and its platelet CD36 receptor10, that act within the platelet–platelet contact zone or ‘synapse’ after the initial aggregation event and ultimately promote thrombus growth and stability11.
A second area of research focus that distinguishes molecular and cellular mechanisms of haemostasis and thrombosis involves heterotypic cell–cell interactions between leukocytes and platelets. Platelet–leukocyte interactions induce bidirectional signals that amplify pro-inflammatory and pro-thrombotic cellular responses12. A more complete understanding of the molecular basis of leukocyte–platelet complex formation may provide key insight into candidate anti-thrombotic targets.
Adhesive interactions between vascular cells play important roles in orchestrating the inflammatory response. Recruitment of circulating leukocytes to vascular endothelium requires multistep adhesive and signalling events, including selectin-mediated attachment and rolling, leukocyte activation, and integrin-mediated firm adhesion and diapedesis that result in the infiltration of inflammatory cells into the blood vessel wall13. Firm attachment is mediated by members of the β2-integrin family, LFA-1 (αLβ2, CD11a/CD18), Mac-1 (αMβ2, CD11b/CD18) and p150,95 (αxβ2, CD11c/CD18), and CD11d/CD18 (αDβ2), which bind to endothelial counter ligands (for example, intercellular adhesion molecule-1; ICAM-1), endothelial-associated extracellular matrix proteins (for example, fibrinogen) or glycosaminoglycans14,15.
Leukocyte recruitment and infiltration also occur at sites of vascular injury where the lining endothelial cells have been denuded, and platelets and fibrin have been deposited. A similar sequential adhesion model of leukocyte attachment to and transmigration across surface-adherent platelets has been proposed16. The initial tethering and rolling of leukocytes on platelet P-selectin17 are followed by their firm adhesion and transplatelet migration, processes that are dependent on αMβ2 (ref. 16).
Integrins are heterodimeric proteins composed of one α- and one β-subunit. A subset of integrin α-subunits, including αM, contains an inserted domain (I-domain) of ∼200 amino acids that is implicated in ligand binding18 and is strikingly similar to the A domains of von Willebrand factor (vWF)19, one of which, A1, mediates the interaction of vWF with its platelet receptor, the glycoprotein (GP) Ib–IX–V complex. Because of the similarity of the vWF A1 domain and the αMI-domain, we hypothesized that GPIbα might also be able to bind αMβ2 and reported that GPIbα is indeed a constitutively expressed counterreceptor for αMβ2 (ref. 20).
The αMI-domain contributes broadly to the recognition of ligands by αMβ2 (ref. 18) and specifically to the binding of GPIbα (ref. 20). This region has also been implicated in the binding of many ligands, including ICAM-1 (ref. 21), C3bi (ref. 22) and fibrinogen21. We localized the binding site for GPIbα within the αMI-domain segment αM(P201–K217) using a strategy based on the differences in the binding of GPIbα to the αMI- and αLI-domains that involved several independent approaches, including screening of mutant cells, synthetic peptides, site-directed mutagenesis and gain-in-function analyses23. Antibody targeting of αM(P201–K217) blocked αMβ2-dependent adhesion to GPIbα, but not several other ligands and inhibited leukocyte accumulation, cellular proliferation and neointimal thickening after arterial injury24, and broadly regulated the biological response to tissue injury in models of vasculitis25, glomerulonephritis26 and experimental autoimmune encephalomyelitis27.
Since leukocyte–platelet interactions bidirectionally induce signals that amplify pro-inflammatory and pro-thrombotic cellular responses12, we hypothesized that leukocyte Mac-1 engagement of platelet GPIbα is critical for thrombus formation. In this study utilizing genetic, antibody, and small-molecule approaches, we provide evidence that Mac-1:GPIbα directly modulates thrombosis without influence on tail bleeding time or other haemostatic parameters.
Carotid artery thrombosis is delayed in Mac-1 −/− mice
To elucidate the effect of Mac-1 on the development of arterial thrombosis in real-time, carotid arteries of wild-type (WT) and Mac-1−/− mice were subjected to the Rose Bengal model of thrombosis, an endothelial cell photochemical injury model due to local free radical release28,29. Carotid artery blood flow was then monitored continuously with a vascular flow probe. Mean time to occlusive thrombus formation in WT mice was 21.7±6.4 min, and was prolonged significantly in Mac-1−/− mice to 60.8±20.4 min (n=7–13 per group; Fig. 1a).
Impaired thrombus formation in Mac-1 −/− microvasculature
The cremaster thrombosis model was implemented to examine the influence of Mac-1 in a small vessel arteriole as contrasted to the large vessel carotid artery used in the Rose Bengal model. Thrombus formation after laser-induced injury to the arteriolar wall in the cremaster microcirculation of Mac-1−/− mice was compared with that of WT mice, using intravital microscopy30. In WT mice, platelet accumulation in arterioles was evident within 15 s of laser injury and increased progressively over the 90 s observation period (Fig. 1b). In contrast, platelet accumulation was markedly attenuated in Mac-1−/− mice. Analysis of the growth curves of continuous, real-time thrombus profiles assessed by integrated fluorescence intensity of labelled platelets over time showed marked attenuation of platelet thrombus growth in Mac-1−/− mice (WT: 14.8±14.6 × 106 arbitrary fluorescent units (a.u.) versus Mac-1−/−: 4.5±5.1 × 106 a.u., n=33–35 arterioles per group; Fig. 1c,d). Mean % inhibition over time was 70.0%. Initial platelet adhesion and small platelet aggregates were observed in Mac-1−/−mice, but developing thrombi were unstable and embolized frequently.
Similar platelet count and coagulation assays in WT and Mac-1 −/− mice
Having observed delayed thrombosis in Mac-1−/− mice, we set out to determine the mechanism by first performing screening platelet and coagulation assays in WT and Mac-1−/− mice. We performed complete blood count on whole blood from WT and Mac-1−/− mice (Supplementary Table 1). White blood cell count (Supplementary Table 1) and platelet count were similar in WT (786,400±317,800 platelets per μl, n=5) and in Mac-1−/− (775,700±176,000 platelets per μl, n=6) mice (Fig. 2a). Coagulation activity of plasma was assessed using the activated partial thromboplastin time (aPTT) and a thrombin generation assay. The aPTT was not prolonged in Mac-1−/− mice (WT: 66±28 s versus Mac-1−/−: 46±11 s; Fig. 2b). Tissue factor (TF)-induced total thrombin generation was not reduced in Mac-1−/− plasma (WT: 21,055±407 versus Mac-1−/−: 22,398±830 a.u., n=4 per group; Fig. 2c). Taken together, these data indicate that neither platelet count nor coagulation parameters likely account for delayed thrombosis in Mac-1−/− mice.
Unimpaired platelet activation and signalling in Mac-1 −/− platelets
Although leukocyte-restricted expression of Mac-1 makes it unlikely that defective thrombus formation in Mac-1−/− mice is due to an intrinsic platelet activation defect, we nonetheless assessed platelet activation in platelets isolated from WT and Mac-1−/− mice by monitoring the expression of P-selectin and activated αIIbβ3 (GPIIb/IIIa) in response to agonist stimulation. Washed platelets from WT and Mac-1−/− mice were stimulated with collagen, thrombin or arachidonic acid. Platelet activation as measured by both P-selectin expression (Wug.E9-positive staining) and activated αIIbβ3 (JON/A-positive staining) is similar in Mac-1−/− platelets compared to WT platelets in response to the treatment of thrombin (Supplementary Fig. 1a,b), collagen (Supplementary Fig. 1c,d) or arachidonic acid (Supplementary Fig. 1e,f). In addition, we demonstrated there was no difference in platelet adhesion (Supplementary Fig. 1g) and spreading on collagen (Supplementary Fig. 1h) between WT and Mac-1−/− mice.
Transfer of WT leukocytes restores thrombosis defect in Mac-1 −/− mice
Although we have provided evidence that deficiency of Mac-1 is associated with prolonged time to carotid artery occlusion after photochemical injury, we have utilized mice with global rather than tissue- or cell-specific deficiency of Mac-1, thereby limiting our ability to conclude definitively that leukocyte Mac-1 is critical for thrombus formation. To address this issue, we performed adoptive transfer experiments of WT and Mac-1−/− donor peripheral blood mononuclear cells (PBMCs) or neutrophils into Mac-1−/− recipient mice before photochemical injury. Mac-1−/− recipient mice that received Mac-1−/− donor PBMCs formed occlusive thrombi in 49.8±17.2 min (Fig. 3a). Strikingly, the time to occlusive thrombus formation was shortened significantly in Mac-1−/− recipient mice receiving WT donor PBMCs to 26.6±6.9 min (Fig. 3a), nearly restoring occlusion time to that observed in WT mice (21.7±6.4 min; Fig. 1a).
We also performed adoptive transfer of WT or Mac-1−/− neutrophils isolated by density gradient centrifugation into Mac-1−/− recipient mice. Mac-1−/− mice that received Mac-1−/− donor neutrophils formed occlusive thrombi in 57.2±18.7 min. The time to occlusive thrombus formation was significantly shortened in Mac-1−/− recipient mice that received WT donor neutrophils to 29.6±15.7 min (Fig. 3b). Taken together, these adoptive transfer experiments indicate that Mac-1 on either PBMCs or neutrophils contributes to arterial thrombus formation.
Mac-1 signalling regulates TF via transcription factor Foxp1
Having demonstrated the importance of leukocytes in thrombosis, we next sought to elucidate the underlying mechanism. Platelet–leukocyte interactions bidirectionally induce signals that amplify pro-inflammatory and pro-thrombotic cellular responses12. Previous work from our laboratories has demonstrated that leukocyte engagement of platelet GPIbα via Mac-1 induces platelet ‘outside-in’ signalling and platelet activation31. We next asked whether leukocyte engagement of platelet GPIbα via Mac-1 is capable of inducing ‘outside-in’ Mac-1 signalling by evaluating phosphorylation of protein kinase C (PKC) and expression of Foxp1. We and others have reported that Mac-1 clustering by fibrinogen triggers phosphorylation and activation of PKC delta that, in turn, regulates expression of the transcription factor Foxp1 (refs 32, 33). Indeed, clustering of Mac-1 by GPIbα induced phosphorylation of PKC delta (Fig. 4a), and downregulated Foxp1 expression (Fig. 4b).
Foxp1 functions as a transcriptional repressor, and we have shown that downregulation of Foxp1 is required for monocyte differentiation and macrophage function in vitro and in vivo32,34. We hypothesized that Mac-1 may regulate thrombosis via Foxp1 and TF. We turned our attention to TF because TF initiates arterial thrombus formation in response to laser-induced injury of endothelial cells35,36. We first analysed the levels of TF in PBMCs isolated from WT and Mac-1−/− mice. The expression of TF is reduced in Mac-1−/− compared to WT leukocytes (Fig. 4c). To investigate whether TF expression is influenced by Mac-1–Foxp1 signalling, mouse NIH/3T3 cells were co-transfected with the TF promoter reporter gene plasmid, pRSV-β-gal, and expression plasmids for Foxp1 or pcDNA3.1 vector control. Overexpression of Foxp1 significantly inhibited TF promoter activity in unstimulated (% inhibition=66) and phorbol 12-myristate 13-acetate-stimulated (% inhibition=78) cells (Fig. 4d).
To determine whether Mac-1–Foxp1 signalling plays a critical role in regulating thrombosis in vivo, we subjected mice with monocyte-/macrophage-specific overexpression of Foxp1 (macFoxp1tg)34 and WT control mice to carotid artery photochemical injury. Enforced overexpression of Foxp1 significantly prolonged the time to occlusive thrombus formation from 25.0±4.1 min in WT control to 50.1±16.5 min in macFoxp1tg mice (n=11–12 per group; Fig. 4e). Interestingly, TF expression was reduced in Mac-1−/− compared to WT mice (Supplementary Fig. 2). Hence, the prolonged occlusion time in the Mac-1−/− mice can be attributed, likely in part, to increased Foxp1 expression and, consequently, reduced TF expression.
Haemostasis is unimpaired in Mac-1 −/− mice
To assess the role of Mac-1 in haemostasis, we examined tail vein bleeding times. When placing the transected tail tip into a beaker containing saline at 37 °C and then determining the time to complete cessation of bleeding, there was no difference in tail bleeding times between WT and Mac-1−/−mice using either complete cessation of bleeding for 3 min or 30 s as the criteria for bleeding time determination. Mean bleeding time for WT mice was 244±173 s compared to 285±151 s for Mac-1−/− mice (n=9 per group) when complete absence of bleeding for 3 min was the end point (Fig. 5a). With a shorter bleeding cessation period of 30 s, the bleeding time in Mac-1−/− mice was also similar to that in WT mice (76±44 versus 64±44 s; Fig. 5b). Similarly, when blotting the transected tail tip with filter paper and then determining the time to complete cessation of bleeding, there was no difference in tail bleeding times between WT and Mac-1−/− mice. Mean bleeding time for WT mice was 482±145 s compared to 538±207 s for Mac-1−/− mice (n=7–8 per group; Fig. 5c).
Mac-1 and GPIbα interaction is critical for regulation of thrombosis
Mac-1, the most abundant β2-integrin on neutrophils and monocytes, is a highly promiscuous receptor, capable of binding a broad repertoire of ligands (reviewed in ref. 15) and facilitating key leukocyte functions, including migration, coagulation, proteolysis, phagocytosis, oxidative burst and signalling14,37,38,39,40. Elegant structural studies by several groups have begun to elucidate the molecular basis for such broad ligand recognition by Mac-1. A subset of integrin α-subunits, including αM of Mac-1, contains an inserted domain (I-domain) of ∼200 amino acids that is implicated in ligand binding. The αMI-domain contributes broadly to the recognition of ligands by αMβ2 (refs 18, 41), and the binding sites for C3bi, neutrophil inhibitory factor, fibrinogen and GPIbα have been mapped extensively23,42,43,44,45,46. These studies suggest that overlapping, but not identical, sites are involved in the recognition of C3bi, fibrinogen, neutrophil inhibitory factor and GPIbα (refs 23, 47). We reported previously that the P201–K217 sequence, which spans an exposed loop and amphipathic α4 helix in the three-dimensional structure of the human αMI-domain, was a binding site for GPIbα (ref. 23). Site-directed mutagenesis of the P201–K217 sequence within the human αMI-domain allowed us to further narrow the binding region to H210–K217 and subsequently identified two single mutants showing reduced binding to GPIbα (T213 and R216). Indeed, grafting these two critical amino acids onto αL (G213T and N216R) converted αLβ2 into a GPIbα-binding integrin. Thus, the P201–K217 sequence within the αMI-domain is necessary and sufficient for GPIbα binding. Importantly, this site appears to be highly selective for the binding of GPIbα since antibody targeting the P201–K217 sequence inhibited the binding of GPIbα, but not other Mac-1 ligands, including fibrinogen, ICAM-1 and junctional adhesion molecule-3 (JAM-3).
Guided by the identification of the Mac-1-binding site for GPIbα, we took steps towards the generation of a mutant mouse with a double alanine substitution corresponding to the homologous murine sequence S213A and R216A (referred to as muMac-1 mice; Supplementary Fig. 3). We first confirmed that the GPIbα specificity requirement of human αMI-domain also applied to purified murine αMI-domain. WT and mutant murine αMI-domains were expressed in Escherichia coli as gluthatione S-transferase (GST) fusion proteins and purified for use in ligand-binding assays. The E. coli-expressed αMI-domain has been used in multiple functional studies from our laboratories45,48 and from other investigators49. WT αMI-domain (S213 and R216), but not the S213A/R216A αMI-domain double mutant, bound to soluble GPIbα (Fig. 6a). Importantly, the binding of multiple other Mac-1 ligands, including ICAM-1, iC3b, CD40 ligand (CD40L) and fibrinogen, was unaffected by mutation of these two amino acids required for GPIbα binding (Fig. 6b), indicating that the murine S213A/R216A αMI-domain mutant functions similarly to human αMI-domain mutants (T213A/R216A) that we characterized previously23. We also characterized the binding of fluorescent-labelled WT αMI-domain (S213 and R216), single αMI-domain mutants (S213A or R216A) and double αMI-domain mutants (S213A/R216A) to mouse platelets that abundantly express GPIbα. WT αMI-domain (S213 and R216) bound to mouse platelets and this binding was reduced with both single and double αMI-domain mutants (Fig. 6c). The residual binding of the αMI-domain double mutant (S213A/R216A) to platelets may reflect its binding to other platelet surface ligands, such as JAM-3 (ref. 50) or heparin/heparan sulfate51.
To determine whether Mac-1 regulates thrombosis through its interaction with platelet GPIbα rather than other ligands, we subjected muMac-1 mice to carotid artery photochemical injury (Fig. 7a). The mean time to occlusive thrombus formation was prolonged significantly in muMac-1 (44.8±27.6 min) compared with WT mice (27.0±10.6 min). Importantly, we verified that complete blood count of whole blood from muMac-1 mice was similar to that of WT mice (Supplementary Table 1), and that platelet activation in response to agonist stimulation (that is, expression of P-selectin and activated αIIbβ3) was unaffected in platelets isolated from muMac-1 compared to WT mice (Supplementary Fig. 4). Platelet adhesion (Supplementary Fig. 1g) and spreading (Supplementary Fig. 1h) on collagen were unimpaired in muMac-1 mice. Next, we examined haemostasis in muMac-1 mice. There was no difference in tail bleeding time between WT and muMac-1 mice (mean bleeding time WT: 69±35 s versus muMac-1: 65±29 s, n=8–9 per group; Supplementary Fig. 5a). Finally, key leukocyte functions, including migration (as assessed by peritoneal macrophage accumulation after thioglycolate-induced peritonitis) and phagocytosis of Red Zymosan fluorescent beads, were unaffected in muMac-1 mice (Supplementary Fig. 5b,c,d).
Thrombus formation after laser-induced injury to the arteriolar wall in the cremaster microcirculation of muMac-1 mice was also compared with that of WT mice, using intravital microscopy30. In WT mice, platelet accumulation in arterioles was evident within 15 s of laser injury and increased progressively over the 90 s observation period; in contrast, platelet accumulation was markedly attenuated in muMac-1 mice (Fig. 7b). Analysis of the growth curves of continuous, real-time thrombus profiles assessed by integrated fluorescence intensity of labelled platelets over time showed marked attenuation of platelet thrombus growth in muMac-1 mice (WT: 41.3±52.7 × 106, n=16 arterioles versus muMac-1: 4.6±6.6 × 106, n=31 arterioles; Fig. 7c,d). Mean % inhibition over time was 89%. Taken together, these observations indicate that Mac-1-GPIbα regulates both large vessel and small vessel arterial thrombosis.
Antibody targeting Mac-1:GPIbα inhibits thrombus formation
Having established a role for Mac-1 and its interaction with platelet GPIbα in thrombosis using genetic approaches, we next investigated the effect of antibody targeting of Mac-1:GPIbα interaction on thrombosis. We have reported previously on the generation of an antibody targeting αMI-domain P201–K217 (termed anti-M2) that selectively blocks the binding of Mac-1 to GPIbα, but not to other Mac-1 ligands24. This antibody attenuates inflammation and tissue injury in a variety of animal models, including restenosis24, vasculitis25, glomulerulonephritis26 and experimental autoimmune encephalomyelitis27. Anti-M2 (100 μg via tail vein) was injected into mice before photochemical carotid artery injury. Strikingly, antibody targeting of Mac-1:GPIbα prolonged significantly the time to occlusive thrombus formation to 70.2±16.8 min in anti-M2-treated mice compared to 23.5±2.1 min in control IgG-treated mice (Fig. 7e).
Small-molecule screen for inhibitors of Mac-1:GPIbα binding
An antibody raised to the M2 peptide sequence in the αMI-domain of integrin blocks binding of GPIbα and platelets to the integrin and to leukocytes24. The anti-M2 antibody blocks Mac-1:GPIbα binding, but does not inhibit binding of other Mac-1 ligands. This behaviour suggests that small-molecule inhibitors of Mac-1:GPIbα might be developed for therapeutic utility. We have taken the initial steps to identify lead compounds with such blocking activity. We tested the 2,000 compounds in Spectrum collection from Microsource.
For initial screening of the library, we tested the compounds at a 100 μM concentration as inhibitors of binding recombinant fluorescently labelled αMI-domain to Chinese hamster ovary (CHO) cells expressing GPIbαβ. A representative screening assay showing the differential activity of 10 consecutive compounds tested, including both positive and negative hits, is shown in Supplementary Fig. 6a. Altogether, we obtained 97 positive hits, which inhibited the interaction by about 50% and then retested these at concentrations of 10, 30 and 50 μM. Eliminating those compounds that did not inhibit or were inhibitory at a single concentration reduced the number of compounds to 50. Of these, we moved forward with 36 compounds that were readily available.
Several approaches were developed to further characterize and select among the 36 positive hits. As negative selection criteria, we excluded compounds that caused clumping of neutrophils and platelets. As a specificity control, we excluded compounds that inhibited the adhesion of HEK-293 cells expressing Mac-1 to immobilized fibrinogen, another ligand of the integrin. As positive controls, we measured direct binding of the compounds to αMI-domain or to GPIbα in surface plasmon resonance (SPR) experiments. Compounds in both categories were identified, and several bound at low micromolar to sub-micromolar concentration.
Four more sets of assays have been performed subsequently: (1) SPR to determine which compounds interacted with the I-domains of four β2-integrins, αLβ2, αMβ2, αXβ2 and αDβ2; (2) inhibitory activities of the compounds on adhesion of HEK-293 cells expressing αMβ2 to CHO cells expressing GPIbα; (3) effects of the compounds on the interaction of naturally occurring cells: inhibition of human platelet phagocytosis by human neutrophils; and (4) binding of labelled αMI-domain to human platelets was assessed, an assay that allowed us to assess the potency of the compounds as inhibitors of platelet–integrin interaction.
On the basis of these assays, a group that bound specifically to the αMI-domain was identified. A representative of this group was glucosamine, which we explored in further in vitro and in vivo experiments. In SPR experiments, WT and αMI-double mutant were immobilized on CM5 chips, and binding of glucosamine to the surface was monitored in a BiaCore 3000 instrument. Under the conditions used, while glucosamine bound to WT αMI-domain (Fig. 8a, left) in a concentration-dependent manner, no consistent interaction of the sugar derivative with the αMI-double mutant was detected (Fig. 8a, right). Because of the low signal obtained not only with the αMI-double mutant but also with the WT αMI-domain, we did not attempt to derive binding constants from these data. The literature indicates that evaluation of carbohydrate binding by SPR can be challenging52. Hence, we increased the coating density of the WT and αMI-double mutant on the chip from ∼2,500 relative units (RU) on the chip to ∼6,000 RU on the CM5 chip surface. Under this condition, we detected low-level binding of both WT αMI-domain and the αMI-domain double mutant (Supplementary Fig. 7) although the responses obtained with WT αMI-domain was consistently greater. In attempt to derive a binding constant, we used a steady-state approach to interpret the data (Fig. 8b), an approach found to be useful for analysis of progress curves from low-affinity interactions52. The binding isotherm for WT αMI-domain yielded an estimated Kd of ∼100 μM, whereas that of the αMI-double mutant was ∼244 μM. This difference indicates that one site of glucosamine binding is influenced by S213A/R216A mutation. Independent approaches were implemented to verify that glucosamine inhibits the interaction of αMI-domain with GPIbα. First, binding of biotinylated GPIbα to αMI-domain immobilized on microtitre plates was detected with streptavidin–horseradish peroxidase (HRP) conjugate. This interaction was inhibited in a dose-dependent manner by glucosamine (Fig. 8c). The concentration of glucosamine inhibiting binding by 50% (IC50) was ∼50 μM, approximating the Kd estimated from the SPR experiments. Second, an assay in which binding of Alexa-488-labelled Mac-1-expressing 293 cells to adherent GPIbα-transfected CHO cells was developed. This interaction was inhibited by an anti-Mac-1 antibody, by an anti-GPIbα antibody or by glucosamine (Fig. 8d). Indeed, in this assay, glucosamine produced dose-dependent inhibition (Fig. 8e). We also compared the specificity of glucosamine to several similar carbohydrate derivatives (Supplementary Fig. 6b). Of these compounds, only glucosamine produced significant inhibition of GPIbα binding to the αMI-domain (Supplementary Fig. 6b).
To better understand how glucosamine interacts with αMI-domain, we performed docking analysis to calculate the potential binding mode of glucosamine by using Schrödinger Maestro software. Multiple possible conformations were generated by defining R216 as potential binding site. One conformation with best docking score of ‘−4.053’ was selected. In this binding mode, glucosamine binds to a small pocket of αMI-domain formed by the α-helix residues from T211 to E221 (Fig. 9a). It is spatially close to T213 and forms several critical H-bonds with the side chains of R216, K217, R220 and E221 (Fig. 9b). This docking mode provides a basis for understanding our mutagenesis study that showed that T213A/R216A mutant abolished the glucosamine binding. In comparing the conformation of glucosamine docked in this model, the root mean squared deviations in the eight next best fits were all quite similar, varying from −0.026 to −0.093, to that shown in Fig. 9a.
The anti-thrombotic potential of glucosamine as an inhibitor of Mac-1:GPIbα binding was then investigated in the carotid artery photochemical injury model. Glucosamine (27 μg) or phosphate-buffered saline vehicle control were administered via tail vein injection immediately before carotid artery injury. The small-molecule Mac-1:GPIbα inhibitor glucosamine significantly prolonged thrombus formation to 53.2±15.4 min compared to 24.7±8.4 min for vehicle control (Fig. 7f). We also examined haemostasis in mice treated with glucosamine. There was no difference in tail bleeding time between mice treated with buffer or glucosamine (mean bleeding time buffer: 73±31 s versus glucosamine: 82±35 s, n=12 per group; Supplementary Fig. 5e). Taken together, these observations indicate that genetic, antibody and small-molecule targeting of Mac-1:GPIbα binding are capable of influencing arterial thrombus formation in vivo.
In this study, we have identified a new pathway of thrombosis involving leukocyte Mac-1 and platelet GPIbα, and interfering with this pathway does not affect parameters of haemostasis. This conclusion is supported by the following data: (1) mice with deficiency of Mac-1 (Mac-1−/−) or mutation of the Mac-1-binding site for GPIbα (muMac-1) have delayed thrombus formation after injury to large and small arteries; (2) platelet count, platelet activation, plasma coagulation activity and bleeding time were similar in WT and Mac-1−/− mice; (3) adoptive leukocyte transfer rescued defective thrombus formation in Mac-1−/− mice; (4) Mac-1-GPIbα induces ‘outside-in’ Mac-1 signalling (that is, phosphorylation of PKC and downregulation of Foxp1), and Mac-1-dependent regulation of the transcription factor Foxp1, which regulates TF expression, contributed to the thrombosis defect as evidenced by prolonged thrombotic occlusion time in macFoxp1tg mice; and (5) antibody and small-molecule targeting of Mac-1:GPIbα inhibited thrombus formation.
Platelet–leukocyte interactions bidirectionally induce signals that amplify pro-inflammatory and pro-thrombotic cellular responses12. One of the key implications of our findings is the central importance of leukocyte Mac-1 and platelet GPIbα for leukocyte–platelet interactions in vivo. Other reported interactions contributing to Mac-1-independent leukocyte–platelet conjugate formation include thrombospondins bridging between GP IV receptors on platelets and monocytes53, and P-selectin on activated platelets binding with leukocyte P-selectin glycoprotein ligand-1 (refs 54, 55). However, stable accumulation of leukocytes to adherent platelets ex vivo under experimental conditions of arterial shear or to the endothelial–denuded vessel lined with platelets in vivo, requires leukocyte Mac-1 and platelet GPIbα (ref. 24). Other potential Mac-1 ligands present on the platelet membrane include fibrinogen (bound to αIIbβ3)56,57, ICAM-2 (ref. 58) and JAM-3 (ref. 50). However, a leukocyte–platelet interaction mediated by fibrinogen bridging between Mac-1 and αIIbβ3 has been largely discounted by Ostrovsky et al.59 who found that neither RGDS peptides nor the replacement of normal platelets with thrombasthenic platelets (that is, lacking αIIbβ3) affected the accumulation of the leukocytes on platelets. Although Mac-1 binds ICAM-1, this receptor is not found on platelets. Platelets express a related receptor, ICAM-2 (ref. 58), but Diacovo et al.16 have shown that ICAM-2 blockade has no effect on the firm adhesion of neutrophils on monolayers of activated platelets under flow. Santoso et al.50 have reported that Mac-1 may also bind to platelet JAM-3, cooperating with GPIbα to mediate neutrophil–platelet adhesive contacts in vitro. However, we have reported previously that anti-M2, which is capable of blocking platelet-dependent leukocyte recruitment both ex vivo and in vivo, had minimal inhibitory effect on Mac-1-dependent adhesion to JAM-3 (ref. 24).
Genetic (muMac-1 mice) and antibody approaches were utilized to investigate the importance of Mac-1 binding to GPIbα, but not to other Mac-1 ligands in thrombosis. The relative specificity of anti-M2 inhibitory action towards GPIbα (that is, non-inhibitory towards ICAM-1, fibrinogen, JAM-3 and C3bi) suggests a minor contribution of other ligands for Mac-1 in the context of thrombosis.
Previous work from our laboratories has demonstrated that leukocyte engagement of platelet GPIbα via Mac-1 induces platelet ‘outside-in’ signalling and platelet activation31. We now provide new evidence that engagement of platelet GPIbα via Mac-1 induces ‘outside-in’ Mac-1 signalling that leads to phosphorylation of PKC delta and downregulation of Foxp1 in monocytic cells. Thus, blockade of the initial cell–cell conjugation mediated by Mac-1:GPIbα may prevent bidirectional signalling that amplify thrombus formation, and account for the effectiveness of Mac-1:GPIbα inhibition in reducing thrombus formation in vivo.
Having established that adoptive transfer of WT neutrophils or PBMCs partially corrects the thrombosis defect in Mac-1−/− mice, one needs to consider the possibility that there may be distinct mechanisms driving neutrophil versus mononuclear leukocytes in thrombus formation. While TF may be important in mononuclear cell-dependent thrombosis, it is controversial whether neutrophils express TF. Neutrophils are known to regulate thrombosis through the formation of neutrophil extracellular traps (NETs), which stimulate thrombus formation and coagulation and are abundant in thrombi in animal models of deep vein thrombosis60. The molecular basis of NET generation (known as NETosis) is a complex process requiring reactive oxygen species production61 and neutrophil proteases (that is, neutrophil elastase, myeloperoxidase and peptidylargine deiminase-4)62. Highly relevant to the present study, Neeli et al.63 have provided evidence that the Mac-1 itself may be involved in the initiation of changes in the neutrophil cytoskeleton that facilitate the breakdown of nuclear and plasma membranes for the releases of NETs.
The present observations suggest a possible target for therapeutic intervention in cardiovascular and thrombotic diseases. In particular, the specificity of antibody or small-molecule inhibitory action towards Mac-1:GPIbα suggests that it might be possible to inhibit pro-thrombotic leukocyte–platelet interactions without affecting other Mac-1 functions. Our study identifies glucosamine as one such small-molecule antagonist. The failure of other molecules of similar size and composition to glucosamine to block αMI-domain:GPIbα interaction augers well for the possibility of detailed structure–activity analyses to identify more potent small-molecule antagonists. Our modelling study (Fig. 9) suggests that several closely related binding modes would allow glucosamine to bind in close proximity to T213/R216 and interfere with GPIbα binding. Ultimately, solving the crystal structure of glucosamine or other small molecules identified in our screen or of an anti-M2 bound to the αMI-domain may lead to a new class of anti-thrombotic therapy. At a more fundamental level, the results of this study suggest that thrombosis and haemorrhage may be uncoupled at the level of the Mac-1:GPIbα interaction. In particular, the specificity of antibody or small-molecule inhibitory action towards Mac-1:GPIbα suggests that it might be possible to inhibit pro-thrombotic leukocyte–platelet interactions without affecting other Mac-1 functions. Deficiency of Mac-1 did not interfere with tail bleeding time, platelet activation and plasma coagulation activity (that is, aPTT and thrombin generation). The identification of a new platelet-dependent pathway of thrombosis that does not affect haemostatic parameters, such as bleeding time and platelet adhesion and spreading, has possible clinical implications. Thrombotic cardiovascular diseases, including myocardial infarction and stroke, are the leading cause of death in developed countries1. Total US healthcare expenditures in 2009 for coronary heart disease and stroke were a staggering $165.4 billion and $68.9 billion, respectively1 with pharmacologic therapies estimated to exceed $20 billion worldwide1. Antiplatelet agents and anticoagulants are used in the treatment of acute coronary syndrome and in primary and secondary prevention of coronary artery disease and stroke64,65. Current drugs are subject to significant bleeding risk, which is associated with increased mortality2,3,4. While new antiplatelet (for example, prasugrel, ticagrelor and vorapaxar) and anticoagulant (for example, apixaban, dabigatran and rivaroxaban) agents have been approved on the basis of superior efficacy or other clinical advantages (for example, fixed dosing without the need for monitoring), these therapeutic advances are associated with a 25–30% increase in the rate of bleeding or transfusion. There is emerging experimental evidence distinguishing the molecular and cellular mechanisms of haemostasis and thrombosis5,6. The interaction between leukocyte Mac-1 and platelet GPIbα is now positioned as a novel and targetable mediator of thrombosis, but not haemostasis (that is, reduced bleeding risk).
Antibody to mouse P-selectin/CD62P conjugated to fluorescein isothiocyanate (Wug.E9) and antibody to mouse activated integrin αIIbβ3 (GPIIb/IIIa) conjugated to R-phycoerythrin (JON/A) were purchased from emfret Analytics (Würzburg, Germany, Catalogue #: D200). Polyclonal antibody (termed anti-M2) to the Mac-1-binding site for GPIbα was generated by YenZym Antibodies, LLC (South San Francisco, CA). Antibody to TF was purchased from R&D Systems Inc. (AF3178, Minneapolis, MN). Rose Bengal (4, 5, 6, 7-tetrachloro-3′, 6-dihydroxy-2, 4, 5, 7-tetraiodospiro (isobenzofuran-1(3H), 9 [9H] xanthan)-3-1 dipotassium salt) was purchased from Sigma-Aldrich (St Louis, MO). Human α-thrombin was purchased from Haematological Technologies (Essex Junction, VT, Catalogue # HCT-0020). Collagen (Catalogue # 101562) and arachidonic acid (Cat # 101297) were purchased from Bio/DATA Corporation (Horsham, PA).
All mice had a congenic C57BL/6 background and were maintained in animal facilities at Case Western Reserve University School of Medicine.
Mac-1−/− mice were generated in the laboratory of Dr Christie Ballantyne39. Mutant Mac-1 mice expressing the S213A/R216A double-mutant αMI-domain were generated at Ozgene Pty. Ltd (Bentley, Australia) using Cre-mediated inversion strategy by flanking an inverted exon 7 fragment, containing the knock-in sequence with lox66 and lox71 sites66,67. The following four fragments were generated by PCR from C57BL/6 genomic DNA and cloned into the Ozgene plasmid PacF 10000113-A08: (a) mutant exon 7 fragment (KI)—the KI fragment contained PacI and ClaI sites for cloning, an EcoRV site for genomic screening and a lox71 site at the 3′-end; (b) WT exon 7 fragment (wt)—the wt fragment contained ClaI and AscI sites for cloning and a lox66 site at the 5′-end; (c) 5′-homology arm (5H)—the 5H arm contained AscI and AatII sites for cloning, and NdeI and MfeI sites for genomic screening; and (d) 3′-homology arm (H3)—the H3 arm contained an AatII site for cloning and an NdeI site for genomic screening. The targeting vector containing all four fragments was sequenced and introduced into embryonic stem cells by electroporation. Embryonic stem cells in which homologous recombination occurred as detected by Southern blot analysis were injected into a mouse blastocyst to generate chimeric mice. Offspring of chimera × C57Bl/6 mating confirmed as wt/flox underwent three additional breeding to remove Neo, FLP and Cre cassettes, and to bring the mutated exon 7 into reading frame. Breeding step 1: to remove the selection cassette from a heterozygous wt/flox line by breeding to heterozygous wt/FLP mice. Breeding step 2: to remove the FLP gene and to generate a global Cre inverted wt/KI line by breeding the wt/floxΔneo–wt/FLP line generated in breeding step1, to homozygous Cre mice. Breeding step 3: to remove the Cre gene by breeding the wt/KI—wt/Cre mice generated in step 2, back to C57BL/6J mice. After the establishment of the mutant mouse colony, mice were routinely genotyped by PCR of genomic tail DNA using the following primers in two separate reactions to generate a mutant band of 469 bp (YM121 and YM131) and a WT band of 585 bp (YM121 and YM128): YM121 (5′-GTCCTACCTCGACATGTTCTTTTC-3′); YM128 (5′-AGCATAGGCTTAATCCACCTCTCT-3′); and YM131 (5′-ACACTACTTTGGCGATCCCGGC-3′). macFoxp1tg mice were generated in our laboratory as reported34.
Mouse platelets were isolated from the whole blood obtained by terminal inferior vena cava phlebotomy as described10,68. Briefly, platelet-rich plasma was prepared by centrifugation, and platelets were suspended in Tyrode’s buffer. Platelet suspensions were adjusted to final density after counting particles >3 fl using a Z1 series Coulter Counter (Beckman Coulter, Fullerton, CA) equipped with a 50 μm aperture or were measured as part of a complete blood count of sodium citrate-anticoagulated mouse blood on a HEMAVET 950FS system in the Case Comprehensive Cancer Center, Case Western Reserve University School of Medicine.
Activated partial thromboplastin time
The aPTT was performed using Amelung KC4 coagulation analyser (Sigma, St Louis, MO), as described previously10,69. Briefly, 100 μl of sodium citrate-anticoagulated plasma was incubated with 50 μl of aPTT reagent (Siemens, Washington DC) at 37 °C for 5 min. A volume of 50 μl of 30 mM calcium chloride was then added and the time to clot formation was recorded.
TF-induced thrombin generation time was performed, as previously described10,70. Briefly, a 1:2 dilution of mouse plasma was incubated with ∼3 pM TF (3 μl of 1:60 dilution of stock Innovin, Siemens) and 0.42 mM Z-Gly-Gly-Arg-AMC. The reaction was initiated with the injection of 0.16 M calcium chloride, final concentration 16 mM. Substrate hydrolysis was measured on a fluorescent plate reader (NOVOstar, BMG Labtech). The thrombin generation data are expressed as an arbitrary rate of fluorescent accumulation as determined by the second derivative of the raw fluorescent values. The lag time, peak height and total area under the curve were calculated using Prism software (Graphpad, San Diego, CA).
Platelet α-granule release and GPIIb/IIIa activation
Platelet activation assay was performed as previously described10. Briefly, mouse platelets were stimulated for 10 min at room temperature, with agonists. The Wug.E9 and JON/A antibodies were added to detect the expression of P-selectin (CD62P) and activated αIIbβ3 (GPIIb/IIIa), respectively, following the instructions of the manufacturer. After 20 min, platelets were fixed for fluorescence-activated cell sorting (FACS) analysis by addition of formaldehyde. Platelets were distinguished on the basis of side- and forward-light scatter, and the mean fluorescence intensity of platelets was measured using FACSDiva LSRII (Becton Dickinson) and analysed using FACS Diva 6.2 or FlowJo v10.
Photochemical carotid artery thrombosis
This thrombosis model was performed, as previously described10. Briefly, 7- to 9-week-old male mice were anaesthetized and placed on a dissecting microscope (Leica S4E, Leica Microsystems, IL, USA). A midline surgical incision was made to expose the right common carotid artery, and a Doppler flow probe (MC 0.5PSL Nanoprobe, Model 0.5 VB, Transonic Systems, Ithaca, NY) was placed under the vessel. The probe was connected to a flowmeter (Transonic Systems Model TS420) and was interpreted with a computerized data acquisition programme (Windaq, DATAQ Instruments, Arkron, OH). Rose Bengal was injected into the tail vein to administer a dose of 50 mg kg−1 (refs 28, 29). The mid portion of the common carotid artery was then illuminated with a 1.5 mW green light laser source (540 nm; Melles Griot, Carlsbad, CA) 5 cm from the artery. Blood flow was monitored continuously from the onset of injury. The time to occlusion, determined only after the vessel remained closed with a cessation of blood flow for 10 min, was recorded. In a separate group of animals, 100 μg of anti-M2 antibody or 27 μg of glucosamine was also infused into mice via tail vein injection to determine the effect of these GPIbα- and Mac-1-blocking reagents on thrombus formation.
Laser injury to microcirculation using intravital microscopy
Thrombosis was induced, as previously described in male mice aged 11–12 weeks10,30. Briefly, thrombus formation in vivo after laser-induced injury to the arteriolar wall in the cremaster microcirculation of WT was compared with that of Mac-1−/− mice using intravital microscopy (VIVO, 3I Inc.) performed as described previously30. Platelets were labelled in vivo using a fluorescein isothiocyanate--conjugated rat anti-mouse CD41 antibody (BD Pharmingen, San Jose, CA) at a dose of 0.4 μg per g body weight of mouse.
Adoptive transfer experiments
Blood from the inferior vena cava of two mice was collected directly into 3.8% sodium citrate (9:1 blood:citrate) and diluted with equal amount of Tyrode’s buffer. PBMCs were isolated using histopaque (Catalogue #: Histopaque-1077, Sigma-Aldrich, St Louis, MO, USA). Wright-Giemsa staining showed that monocytes represented up to 70% of the PBMC population. Neutrophils were isolated from anticoagulated and diluted blood using Percoll (P1644, Sigma-Aldrich) density gradient centrifugation method. Wright-Giemsa staining showed >85% purity of neutrophils.
Mouse bleeding times
Tail bleeding times were measured by transecting the tails of sex (male and female)- and age (2–3 months old)-matched anaesthetized mice 5 mm from the tip, as previously described10,69. The transected tail tip was placed into a beaker containing saline at 37 °C and the time to complete cessation of bleeding for 30 s and 3 min was determined with a stopwatch. Alternatively, the transected tail tip was blotted with filter paper every 15 s and the time to complete cessation of bleeding was determined with a stopwatch.
TF reporter assay
NIH/3T3 cells were co-transfected with 50 ng of pCMV-β-gal, 0.5 μg of human TF promoter-luciferase and 3.0 μg of pcDNA3.1 vector or pcDNA3.1/FOXP1 construct DNA by Lipofectamine 3000 transfection reagent (Thermo Fisher Scientific, Waltham, MA). Two days after transfection, some samples were treated with 20 nM phorbol 12-myristate 13-acetate for 16 h. Cells were then lysed by 1 × reporter buffer (Promega, Madison, WI) and measured for firefly luciferase activity using Luciferase Assay System reagents (Promega) in a GloMax Microplate Luminometer (Promega). β-galactosidase activity was measured by Enhanced Beta-gal Assay Kit (Genlantis, San Diego, CA). Duplicate measurements of triplicate wells for each sample were performed and the TF promoter-luciferase activities were normalized by the activity of the β-galactosidase internal control.
Mac-1 clustering and signalling
Mac-1-expressing THP-1 monocytic cells were pre-treated with transforming growth factor-β1 (1 ng ml−1) and 1,25-(OH)2 vitamin D3 (50 nM) overnight at 37 °C. Six-well plates were coated with full-length soluble GPIbα (R&D) or N-terminal GPIbα (GC300) for 2 h at room temperature, then blocked by 0.1% polyvinylpyrrolidone (PVP, Sigma) at 37 °C for 1 h. Wells coated with PVP alone were used as control. THP-1 cells were treated with the β2-integrin-activating monoclonal antibody (mAb) KIM185 (10 μg ml−1) and then added to wells coated with full-length GPIbα or N-terminal GPIbα (GC300) to induce Mac-1 clustering and adhesion. After incubation for 2 h at 37 °C, adherent cells (Mac-1-clustered) or non-adherent cells exposed to PVP control wells (non-clustered) were collected, washed and lysed in 1 × RIPA buffer. Protein concentrations were determined by BCA assay, and protein samples (20 μg per lane) were resolved on 4–12% NuPAGE gel for western blot by anti-Phospho-PKC delta (tyr311) antibody (10 μl per 10 ml reaction, Catalogue #: 2055, Cell Signaling Technology). The membrane was re-blotted using anti-total PKC delta (10 μl per 10 ml reaction, Catalogue # ab182126, Abcam) and anti-β-actin (1 μg ml−1, Catalogue # A1978, Sigma-Aldrich) antibodies. Bands were visualized with HRP-conjugated secondary antibody followed by the enhanced chemiluminescence western blotting detection system (PerkinElmer Life and Analytical Sciences, Waltham, MA). For experiments evaluating the effect of Mac-1 clustering on the expression of Foxp1, THP-1 cells were added to wells pre-coated with 0.1% gelatin and gel-filtered human platelets or gelatin-coated wells alone overnight at 37 °C. Cells were then collected as above for immunoblotting with anti-Foxp1 antibody (1 μg ml−1, customer-designed polyclonal antibody raised against CDHDRDYEDEPVNEDME by Zymed Laboratories Inc., South San Francisco, CA) as described previously34.
Thioglycolate-induced peritonitis and isolation of macrophages
Peritonitis was induced in 12- to 20-week-old mice by intraperitoneal injection of 1 ml sterile 3% (wt/vol.) thioglycolate broth. At 48–72 h, peritoneal cavities were lavaged by injecting 10 ml sterile PBS buffer twice with gentle abdominal massage. Leukocytes in the lavaged fluid were counted and macrophages were enriched after brief adhesion to tissue culture plastic to remove non-adherent lymphocytes, resulting in >95% macrophages.
Live functional (adherent) peritoneal macrophages collected using the above method were aliquoted onto two 96-well plates for phagocytosis assay. Macrophages in one 96-well plate were stimulated by lipopolysaccharide (10 μg ml−1) for 24 h, followed by incubation with sonicated pHrodo Red Zymosan, a bioparticle fluorescent beads (from ThermoFisher Scientific), for 2 h at 37 °C. Cells on another plate were stained by BCECF to count seeded/treated live cells for further calibration of phagocytic cell number. The fluorescence intensity of pHrodo beads and BCECF-treated cells were recorded by fluorescent plate reader (CytoFluor II, PerSeptiveBiosystems). Images were captured by EVOS FL (LifeTechnologies).
Expression of recombinant mouse αMI-domains
Mouse αMI-domain was expressed as a GST fusion protein. The coding region of the mouse I-domain (residues E132–A318) was PCR-amplified using the cDNA of murine αM as a template, and the product was cloned into the pGEX-4T-1 expression vector (GE Healthcare Life Sciences, Little Chalfont, UK). The DNA sequence was verified, and the plasmid was used to transform E. coli strain BL-21 competent cells. Expression was induced with 5 mM isopropyl-1-thio-β-D-galactopyranoside (Sigma-Aldrich) for 3–5 h at 37 °C. The fusion protein was purified from the E. coli lysate by affinity chromatography on glutathione–Sepharose (GE Healthcare Life Sciences).
To mutate the residues corresponding to S213 (corresponds to T213 in human αM) and R216 to alanines, site-directed mutagenesis was performed by using the QuikChange II XL Site-Directed Mutagenesis Kit (Agilent Technologies, Santa Clara, CA) according to the manufacturer’s protocol. The pGEX-4T-1 construct containing WT mouse I-domain DNA was modified by PCR using two 52-mer mutagenic primers: 5′-GAATGGGAGGACAAAAACTGCCGCCGGGATCGCAAAAGTAGTGAGAGAACTG-3′ (forward) and 5′-CAGTTCTCTCACTACTTTTGCGATCCCGGCGGCAGTTTTTGTCCTCCCATTC-3′ (reverse). The product was treated with Dpn I endonuclease to digest the parental DNA template, and nicked vector was then transformed into the Gold Ultracompetent XL cells (Agilent) of the E. coli BL-21 strain. Individual bacterial clones were analysed by sequencing, and the presence of the desired mutations and the absence of other mutations in the cloned cDNA were verified. Expression and purification of the mutant I-domains as a GST-fusion protein followed the same procedure as for WT αMI-domain.
Expression of recombinant soluble GPIbα
cDNA encoding amino acids 1–300 of GPIbα was amplified by PCR and cloned into the NheI and XhoI sites of pBIG-4f (ref. 71). CHO Tet-On cells (Clontech, Mountain View, CA) secreting the recombinant GPIbα-300 peptide were incubated for 48 h in serum-free medium (EX-CELL 302; Sigma) containing 10 mM biotin (Sigma) and 2 mg ml−1 doxycycline (Sigma). Conditioned medium was concentrated and desalted to remove free biotin using a PD-10 column (Sigma).
Solid phase assays to test specificity and screen inhibitors
Ligand specificity of WT and mutant murine αMI domains
Wells of Costar 96-well HB plates were coated with 200 μl of 2 μg ml−1 soluble GPIbα, CD40L, iC3b and ICAM-1 (all R&D Systems, Minneapolis, MN), or 1 μg ml−1 human fibrinogen (Enzyme Research Laboratories, South Bend, IN) at 4 °C overnight and 1 h at 37 °C. DH fragment (molecular weight 100 kDa) was prepared by digestion of human fibrinogen with plasmin (Sigma-Aldrich) followed by ion-exchange chromatography on CM-Sephadex and by gel filtration on Sephacryl S-200 (both from Sigma), as described72. Unlike fibrinogen, DH fragment contains an exposed αMβ2 recognition site and supports αMβ2-dependent binding in a dose-dependent manner46. The wells then were post-coated 1 h at 22 °C with 300 μl 0.5% PVP (Sigma-Aldrich). GST-tagged αMI-domains were diluted with Hank’s balanced salt solution (HBSS) containing 20 mM HEPES (pH 7.4), 2 mM CaCl2 and 2 mM MgCl2 (HBSS/HEPES) to 5 μg ml−1 and added to the wells in 200 μl aliquots. As background controls, wells were coated with PVP only. After 1 h incubation at 37 °C, plates were washed with HBSS/HEPES and 200 μl of 5 μg ml−1 anti-GST antibodies conjugated to HRP in HBSS/HEPES, containing 0.5% BSA were added. After 1 h at 37 °C, the plates were washed with HBSS/HEPES, containing 0.1% Tween 80, and 200 μl HRP liquid substrate (Sigma-Aldrich) was added. After 5 min, the reaction was stopped by addition of 50 μl 1 M H2SO4 and absorbance at 450 nm was measured in a multiwell plate reader (Molecular Probes).
Several different variations of microtitre plate assays (96-well TC Costar plates) were used to test inhibitors of αMβ2:GPIbα interaction. In one variation, plates were coated with 150 μl αMI-domain (1 μg ml−1) overnight 4 °C+1 h 37 °C. Plates were post-coated with 200 μl BSA (5 mg ml−1) for 1 h at room temperature and then washed with 150 μl HBSS, containing 20 mM HEPES (pH 7.2), 2 mM CaCl2 and 2 mM MgCl2 (HBSS/HEPES). Anti-αM mAb M1/70, anti-M2 peptide, glucosamine or related carbohydrates at the indicated concentrations were added. Plates were incubated for 20 min at 22 °C, and then 3 μl of GPIbα–biotin conjugate (0.25 mg ml−1) were added. After 30 min at 37 °C, the plates were washed with HBSS/HEPES, and 150 μl streptavidin–HRP conjugate was added. After 30 min at 37 °C the plates were washed with HBSS/HEPES. Bound GPIbα was detected using 3,3′,5,5′-tetramethylbenzidine liquid substrate (Sigma), and absorbance was measured at 450 nm.
In another variation, Mac-1-expressing HEK293 cells73 and cells co-expressing the cDNAs for GPIbα and GPIbβ in CHO cells were prepared as described74. Binding of Alexa-488-labelled Mac-1 cells to GPIbα/β cells grown in microtitre plate wells was assessed in the presence of anti-Mac-1 (ICRF44), anti-GPIbα (VM16d) or glucosamine. After 30 min at 37 °C, the plates were washed a minimum of three times and absorbance was read in a microtitre plate reader. A third assay was used to screen the 2,000 small molecules within the Spectrum collection from Microsource. GPIbα/β cells were grown to confluence in microtitre plates. After washing, Alexa-488-labelled αMI-domain (1 μg ml−1) was added together with 100 μM (final concentration) the test inhibitor in HBSS containing 10 μg ml−1 BSA in a total volume of 200 μl aliquots. As background control, wells coated with PVP only. After 30 min at 37 °C, plates were washed with HBSS/HEPES and read in a spectrophotometer; background binding was taken as the absorbance in the presence of mAb (ICRF44). Each test compound was tested in triplicate, and eight wells on each plate were used to determine background, nonspecific binding.
Surface plasmon resonance
Binding of glucosamine to human WT and mutant αMI-domains was assessed in real time by SPR using a Biacore3000 instrument (Biacore, Uppsala, Sweden). The αMI-domains were immobilized on CM5 biosensor chips using the standard amine coupling chemistry according to the manufacturer’s instructions to achieve either a typical (2,500 RU) or higher coating density (6,000 RU). Experiments were performed at room temperature in 10 mM HEPES (pH 7.4) containing 150 mM NaCl and 0.005% surfactant P20 at a flow rate of 25 μl min−1. SPR sensograms were obtained by injecting various concentrations of glucosamine over the immobilized αMI-domain proteins. The chip surfaces were regenerated by injecting a short pulse of 5 mM NaOH. The curves of buffer only and the blank flow cell were subtracted from the binding curves, and the resulting progress curves were analysed in overlay plots using BIAevaluation software (version 4.01, GE Healthcare) or a steady-state approach.
Molecular docking of glucosamine on the αMI-domain
Molecular docking was performed using Maestro 9.9 software (Schrödinger Release 2014-3, Schrödinger, LLC) with the following procedures.
The structure of D-glucosamine in structure data file (SDF) format was downloaded from PubChem (PubChem CID:439213). It was later processed using ‘LigPrep’ module in Maestro. The compound was desalted, and possible ionization states in the pH range of 5.0–9.0 and tautomers were generated by Epik mode in the force field of OPLS_2005.
The coordinates of αMI-domain was derived from the Protein Data Bank (PDB code: 1BHO). Before docking, the protein was processed and refined with ‘Protein Preparation’ module in Maestro.
Docking grid generation
The residue R216 of αMI-domain was used to define the centre of the docking pocket; the scaling factor and the partial charge cut-off of the van der Waals radii were set to 1.0 and 0.25, respectively. This step was done by using ‘Receptor Grid Generation’ module in Maestro.
Prepared glucosamine was docked into the defined binding pocket using SP (standard-precision) and XP (extra-precision) docking modes, respectively. The docking conformation analysis was performed using PyMol (Version 1.3, Schrödinger, LLC).
Data are presented as mean±s.d. Comparisons between groups were performed by unpaired, two-tailed Student’s t-test. Probability values <0.05 were considered significant.
Animal care and procedures were reviewed and approved by the Case Western Reserve University School of Medicine Institutional Animal Care and Use Committees and performed in accordance with the guidelines of the American Association for Accreditation of Laboratory Animal Care and the National Institutes of Health.
The data supporting the findings of the current study are available from the corresponding author on reasonable request.
How to cite this article: Wang, Y. et al. Leukocyte integrin Mac-1 regulates thrombosis via interaction with platelet GPIbα. Nat. Commun. 8, 15559 doi: 10.1038/ncomms15559 (2017).
Publisher’s note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
This work was supported by National Institutes of Health grants to E.P. (P01HL073311 and R01 HL096062) and D.I.S. (R37 HL57506 and R01 HL126645). We acknowledge Shijian Liu and Xiangru Liang for technical support.
Supplementary Figures and Supplementary Table.
This work is licensed under a Creative Commons Attribution 4.0 International License. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in the credit line; if the material is not included under the Creative Commons license, users will need to obtain permission from the license holder to reproduce the material. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/