<p>Figure S1. Inhibition of Axl by shRNA. Figure S2. Assessment of half maximal inhibitory concentration (IC50) for BGB324 in human CD34+ cells from healthy donors. Figure S3. Treatment with BGB324 increased apoptosis and decreased proliferation of CML cell lines. Figure S4. Reduction of BCR-ABL and Crkl phosphorylation by imatinib. Figure S5. Treatment with imatinib and BGB324 does not induce an additive inhibitory effect on phosphorylation of Erk and Akt. Figure S6. BCR-ABL and Crkl phosphorylation are not affected by imatinib or BGB324 in KCL-22 T315I mutated cells. Figure S7. Colony forming assay using primary CD34+ cells isolated from healthy donors treated for 72 h with 1, 3 or 5 μM of BGB324 (n=2). Figure S8. BGB324 increases apoptosis of primary CML cells.</p>
Summary Temporal and topographic expression of matrix metalloproteinases (MMPs) after perivascular electric injury was studied in wild-type (WT) and urokinase-deficient (u-PA-/-) mice. Neointima formation after injury of the femoral artery was significantly reduced in u-PA-/- mice as compared to WT mice (area of 0.002 ± 0.0007 mm2 versus 0.008 ± 0.002 mm2 at 3 weeks after injury; p <0.001), associated with impaired cellular migration (nuclear cell counts of 44 ± 5 versus 82 ± 9 in cross-sectional areas; p <0.001). Zymographic and/or microscopic analysis indicated that MMP expression gradually increased to reach a maximum at 1 to 2 weeks after vascular injury. In general, MMP levels were lower in u-PA-/- than in WT mice. In non-injured arteries, MMP-2 (gelatinase A) and MMP-3 (stromelysin-1) were produced mainly by adventitial fibroblasts and/or non-contractile smooth muscle cells (SMC). One week after injury, MMP-2 and MMP-3 levels were enhanced due to an increased number and size of producing cells; 2 to 3 weeks after injury, MMP-2 and MMP-3 were produced also by some contractile SMC, which stained with α-actin antiserum. MMP-9 (gelatinase B), MMP-12 (metalloelastase) and MMP-13 (collagenase-3) were found in macrophages located mainly in the adventitia. Immunogold electron microscopic examination revealed that MMP-2 was located predominantly in association with the cell surface of fibroblasts or SMC, while MMP-9 and MMP-12 were located in well defined storage granules within macrophages. MMP-2, MMP-3 and MMP-13, but not MMP-9 or MMP-12, were also found extracellularly, associated with elastin-containing structures (MMP-2), with the basement membrane and occasionally with collagen fibres (MMP-3), or with proteoglycans, collagen and elastin (MMP-13). The temporal and topographic expression pattern of MMPs after vascular injury, coinciding with smooth muscle cell migration and neointima formation, thus is compatible with a role in vascular remodeling.
It is widely held that the plasminogen (Plg) system plays a role in inflammation through plasmin-mediated directional cell migration. However, substantial evidence for its involvement in the inflammatory response has been obtained from indirect studies and lacks firm biological confirmation. To directly characterize plasminogen's involvement in the inflammatory response, we used thioglycollate to induce a peritoneal inflammatory reaction in Plg(+/+),Plg(+/−), and Plg(−/−) mice. At 6 hours poststimulation, neutrophil recruitment into the peritoneum was maximal and similar between Plg(+/+), Plg(+/−), andPlg(−/−) mice. In contrast, monocyte recruitment was significantly diminished after 24 hours poststimulation inPlg(−/−) mice relative to Plg(+/+) mice. Lymphocyte recruitment also was blunted. Blood monocyte levels in these mice indicated that diminished recruitment into the peritoneum was not the result of a diminished source of cells in the circulation. Macrophage phagocytic function was similar between Plg(+/+) and Plg(−/−) mice. This study establishes a direct involvement of plasminogen in monocyte recruitment during a representative inflammatory response.