The JI
HOME HELP FEEDBACK SUBSCRIPTIONS ARCHIVE SEARCH TABLE OF CONTENTS
QUICK SEARCH:   [advanced]


     
 

This Article
Right arrow Abstract Freely available
Right arrow Full Text (PDF)
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Right arrow Citation Map
Services
Right arrow Similar articles in this journal
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Citing Articles
Right arrow Citing Articles via HighWire
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by Russo, S.
Right arrow Articles by Camussi, G.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by Russo, S.
Right arrow Articles by Camussi, G.
Right arrowPubmed/NCBI databases
*Compound via MeSH
*Substance via MeSH
The Journal of Immunology, 2003, 171: 5489-5497.
Copyright © 2003 by The American Association of Immunologists

Platelet-Activating Factor Mediates CD40-Dependent Angiogenesis and Endothelial-Smooth Muscle Cell Interaction 1

Simona Russo*, Benedetta Bussolati*, Ilaria Deambrosis*, Filippo Mariano{dagger} and Giovanni Camussi2,*

* Dipartimento di Medicina Interna e di Scienze Cliniche e Biologiche, Università di Torino and Centro Ricerca Medicina Sperimentale, Ospedale San Giovanni Battista, and {dagger} Dipartimento dell’Area di Medicine, Nefrologia e Unità di Dialisi, Ospedale Centro Traumotologico Ortopedico, Torino, Italy


   Abstract
Top
 Abstract
Introduction
 Materials and Methods
 Results
 Discussion
 References
 
The aim of the present study was to investigate whether stimulation of CD40 expressed by endothelial or smooth muscle cells triggers the synthesis of platelet-activating factor (PAF), an inflammatory mediator with angiogenic properties, and whether PAF contributes to CD40-induced neoangiogenesis. The results obtained indicate that the interaction of CD40 with soluble CD154 or with CD154 expressed on the membrane of leukocytes (CD154-transfected J558 cells) or of activated platelets, stimulated the synthesis of PAF by endothelial cells but not by smooth cells. The synthesis of PAF triggered by activated platelets was inhibited by a soluble CD40-murine Ig fusion protein that prevents the interaction between membrane CD40 and CD154. Studies with specific inhibitors and evaluation of protein phosphorylation indicated the involvement in PAF synthesis of two intracellular signaling pathways leading to cytosolic phospholipase A2 activation: a phospholipase C{gamma}-protein kinase C-Raf-p42/p44-mitogen-activated protein kinase (MAPK) and a MAPK kinase-3/6-dependent activation of p38 MAPK. PAF synthesized by endothelial cells after CD40 stimulation was instrumental in the in vitro migration and vessel-like organization of endothelial cells, and in the interaction between endothelial cells and smooth muscle cells, as inferred by the inhibitory effect of two different PAF receptor antagonists, WEB2170 and CV3988. In vivo, blockade of PAF receptors prevented the angiogenic effect triggered by CD40 stimulation in a murine model of s.c. Matrigel implantation. In conclusion, these observations indicate that PAF synthesis induced by stimulation of endothelial CD40 contributes to the formation and organization of new vessels. This may be relevant in the vascular remodeling associated with tumor and inflammatory neoangiogenesis.


   Introduction
Top
 Abstract
 Introduction
Materials and Methods
 Results
 Discussion
 References
 
A member of the TNF/nerve growth factor receptor superfamily involved in B cell proliferation, differentiation, and survival, CD40 has been recently implicated in the regulation of vascular pathophysiological processes such as atherogenesis (1, 2, 3), tumor neoangiogenesis (4, 5), and inflammation (6, 7, 8). In situ analysis of human atherosclerotic lesions revealed the coexpression of CD154 and CD40 on vascular endothelium and smooth muscle cells (SMC) 3 (1). A direct involvement of CD40 in atherosclerosis was demonstrated by the limiting effect of CD40 inhibition on the evolution of established atherosclerosis in mice (9, 10). Recently, it has also been shown that the engagement of CD40 on endothelial cells by its counterreceptor, the CD154, induces in vitro tubule formation and expression of matrix metalloproteinases, two events involved in neovascularization (11). In vivo, CD40 stimulation has been shown to trigger neoangiogenesis in the model of s.c. Matrigel implantation in mice (5, 12). Moreover, blockade of CD40-CD154 interaction prevented vascularization and growth in an experimental model of Kaposi’s sarcoma (5). We recently found a coexpression of CD40 and CD154 in several renal carcinoma cell lines (13). In these cells, CD40 engagement stimulated cell proliferation, motility, and production of platelet-activating factor (PAF) (13), a phospholipid mediator of inflammation with angiogenic properties (14). PAF is involved in endothelial cell recruitment, and it is critical for the full expression of angiogenic activities of several polypeptide mediators, such as TNF (15) and vascular endothelial growth factor (VEGF) (16).

PAF is thought to be a mediator of cell-to-cell communication, which may function either as an intercellular or an intracellular messenger (17, 18). PAF acts via a specific receptor (PAF-R) (19, 20) coupled with a G-protein, which activates a phosphatidylinositol-specific phospholipase (PL)C (21, 22). The development of potent PAF-R antagonists has allowed investigation of the role of this mediator in cell-to-cell interaction as well as in several pathophysiological conditions (23, 24).

The aim of the present study was to investigate the interaction between CD40-CD154 and PAF-PAF-R systems in two different cell populations involved in the formation of new vessels, the endothelial cells and the SMC. We studied the synthesis of PAF by the endothelial cells and the SMC after stimulation of CD40. Moreover, the role of PAF in the in vitro CD154-induced cell motility, endothelial tube formation, and endothelial-SMC interaction was investigated using two chemically unrelated PAF-R antagonists, WEB2170 and CV3988. In vivo, the role of PAF in CD40-stimulated neoangiogenesis was evaluated in a murine model of s.c. Matrigel implantation after PAF-R blockade with WEB2170.


   Materials and Methods
Top
 Abstract
 Introduction
 Materials and Methods
Results
 Discussion
 References
 
Reagents

M199, DMEM and D-valine-modified MEM, BSA fraction V (tested for <1 ng of endotoxin per milligram), polymyxin B, PLA2, PLA1, EDTA, human thrombin, heparin, trypsin, staurosporine, and FITC-conjugated anti-mouse and anti-rabbit IgG were all purchased from Sigma-Aldrich (St. Louis, MO). FBS and basic fibroblast growth factor (bFGF) were from EuroClone (Wetherby West Yorkshire, U.K.). Recombinant human soluble (s)CD154 trimeric protein, a cross-linking Ab (enhancer) and CD40-murine Ig (muIg) fusion protein, consisting of the extracellular domain of human CD40 fused to mouse IgG2a, were from Alexis Biochemicals (San Diego, CA). Agonist rat anti-mouse CD40 was bought from Serotec (clone 3/23; Oxford, U.K.). Fluorescein-conjugated anti-CD40 and anti-CD154 IgG2a Abs were from EuroClone. Anti-PAF-R polyclonal Abs were obtained from Alexis Biochemicals. Recombinant hirudin, bisindolylmaleimide I and U73122, and SB203580 were purchased from Calbiochem (La Jolla, CA). 4-Bromodiphenacylbromide was from Carlo Erba (Milan, Italy). LY249002 and wortmannin were purchased from Upstate Biotechnology (Lake Placid, NY). Synthetic C16 PAF (1-hexadecyl-2-acetyl-sn-glyceryl-3-phosphorylcholine) was obtained from Bachem Feinchemikalien (Bubendorf, Switzerland). Stock solutions in chloroform were stored at -20°C until use. The chloroform was evaporated, and saline containing 0.25% BSA fraction V, low endotoxin, was added immediately before use. PAF-R antagonist CV3988 (25) was from Takeda Chemical Industries (Kyoto, Japan). PAF-R antagonist WEB2170 (26) was obtained from Boehringer (Ingelheim, Germany). Silica gel 60F254 TLC plates were obtained from Merck (Darmstadt, Germany). µPorasil HPLC columns were provided from the Millipore chromatographic division (Waters, Milford, MA). [3H]Acetate was from NEN Life Science Products (Boston, MA). Growth factor-reduced Matrigel was from BD Labware (Bedford, MA). Rabbit polyclonal anti-phospho-p38 mitogen-activated protein kinase (MAPK), anti-phospho-p42/44 MAPK, and anti-phospho PLC{gamma} Abs, and mouse monoclonal anti-{beta}-actin Ab, all used for Western blot analysis, were obtained from Santa Cruz Biotechnology (Santa Cruz, CA).

Cell lines

HUVEC were isolated by treatment of human umbilical cord veins with 0.5% trypsin (1 h at 37°C) and cultured with M199 with the addition of 20% FBS, 10 ng/ml bFGF and 100 µg/ml heparin until they reached confluence, as previously described (27). They were used at early passages (II–III). Human SMC were isolated from umbilical cords and identified as described (28). CD154-transfected J558L (29) was kindly provided by Dr. A. Mantovani (Istituto Mario Negri, Milan, Italy).

PAF synthesis

In standard PAF synthesis assays, 1 x 106 HUVEC or SMC were maintained for 12 h in DMEM containing 1% FBS. Cells were then equilibrated for 15 min in Tris-buffered Tyrode containing 0.25% delipidized BSA (fraction V), as previously described (15), and incubated at 37°C for the indicated times with the different stimuli. Selected experiments were conducted in the presence of 5 µg/ml polymixin B for 30 min at 37°C to exclude LPS contamination. To obtain CD40 activation, cells were stimulated with recombinant human sCD154 (100 ng/ml). All experiments were performed in the presence of a cross-linking Ab (enhancer, 1 µg/ml). Alternatively, cells were stimulated by a direct coincubation with 1 x 106 J558L stably transfected to express CD154 (29), or J558 cells transfected with only the empty vector. In other experiments, HUVEC were stimulated with activated platelets expressing CD154, according to the protocol of Urbich et al. (30). Briefly, platelets were isolated from full blood of healthy human donors and activated with 0.2 U/ml human thrombin for 5 min at 37°C, and then thrombin was neutralized with 2 U/ml hirudin. Platelets (1.5 x 108) were then coincubated with HUVEC for various times at 37°C. To evaluate the effective CD154 expression of platelets, these cells were characterized by cytofluorimetric analysis. To block the CD154-induced effects, cell were stimulated with sCD154 in the presence of 20 ng/ml CD40-muIg fusion protein. As positive control, HUVEC were stimulated with 1 U/ml human thrombin. For the inhibition experiments, HUVEC were preincubated for 10 min at 37°C with one of the following chemicals: 10 mM EDTA, 1 µM 4-bromodiphenacylbromide, 100 nM staurosporine, 50 µM bisindolylmaleimide I, 10 µM U73122, or 10 µM SB203580.

Extraction and quantification of PAF

The supernatants and the cell pellets were extracted according to a modification of the Bligh and Dyer (31) procedure, with formic acid added to lower the pH of the aqueous phase to 3.0. Each individual experiment was performed in triplicate. PAF was quantified after extraction and purification by TLC (60F254 silica-gel plates; Merck) by aggregation of washed rabbit platelets, as previously reported (15, 27). The biologically active material extracted from cells and supernatants in different experiments was characterized by comparison with synthetic PAF according to the following criteria (15, 27): 1) induction of platelet aggregation by a pathway independent from both ADP and arachidonic acid/thromboxane A2-mediated pathways; 2) specificity of platelet aggregation as inferred from the inhibitory effect of 5 µM WEB2170 or CV3988, two different PAF receptor antagonists (25, 26); 3) TLC and HPLC behavior and physicochemical characteristics, such as inactivation by strong bases and by PLA2 treatment, but resistance to PLA1, acids, weak bases, and 5 min of heating in boiling water. For the radioactive assay of PAF synthesis, 1 x 106 HUVEC were incubated in 1 ml of DMEM for 30 min with 30 µCi of [3H]acetate before each stimulation (16). The cell pellets were extracted according to a modification of the Bligh and Dyer (31) procedure, and lipids were fractionated by TLC on aluminum-sheet silica-gel plates (silica gel 60F254; 0.2-mm thickness; Merck) using a solvent of chloroform/methanol/acetic acid/water (50:25:8:4, v/v/v/v). The plates were cut into 1-cm sections, and the radioactivity of each section was measured. Radiolabeled [3H]PAF (NEN Life Science Products) was used as a standard.

Western blot analysis

After stimulation with sCD154, HUVEC were lysed at 4°C for 15 min in a lysis buffer (150 mM NaCl, 50 mM Tris-HCl (pH 8.0), 5 mM EDTA, 0.1% Igepal, 10 mM sodium fluoride, 10 mM sodium pyrophosphate, 0.4 mM sodium orthovanadate, plus 1 mM PMSF, 10 µg/ml leupeptin, and 100 U/ml aprotinin) and centrifuged at 15,000 x g. The protein contents of the supernatants were measured by the Bradford method. Aliquots containing 50 µg of protein per lane of the cell lysates were subjected to 8 or 12% SDS-PAGE, according to the molecular mass of the protein of interest, under reducing conditions and electroblotted onto nitrocellulose membrane filters. The blots were blocked with PBS plus 0.5% Tween and 10% BSA. The membranes were subsequently immunoblotted overnight at 4°C with the relevant primary Abs or the irrelevant isotypic controls at the appropriate concentration. After extensive washings, the blots were incubated for 1 h at room temperature with peroxidase-conjugated isotype-specific secondary Abs (Santa Cruz Biotechnology), developed with ECL detection reagents (Amersham Biosciences, Arlington Heights, IL) for 2 min, and exposed to X-Omat film (Eastman Kodak, Rochester, NY).

Cytosolic PLA2 (cPLA2) assay

The release of calcium-dependent cPLA2, which exhibits specificity toward arachidonic acid, was measured with an enzymatic assay kit purchased from Cayman Chemicals (Ann Arbor, MI). Briefly, HUVEC stimulated at 37°C for 10 min with sCD154 were detached with a nonenzymatic cell dissociation solution (Sigma-Aldrich), collected, and centrifugated at 1000 x g for 10 min, and then the pellet was sonicated in 1 ml of cold buffer (Tris-HCl containing 50 mM HEPES and 1 mM EDTA, plus 1 mM PMSF, 10 µg/ml leupeptin, and 100 U/ml aprotinin (pH 7.4)). After centrifugation at 10,000 x g for 15 min at 4°C, the supernatants were freezed at -80°C, and an amount was used for the assay kit according to the manufacturer’s protocol.

In vitro cell migration

A total of 1 x 105 cells/well were plated and rested for 12 h in DMEM containing 1% FBS, and then washed three times with PBS and incubated with DMEM containing 0.25% BSA and the agonists. For inhibition studies, in a selected experimental group, cells were previously incubated with WEB2170 (5 µM), or with CV3988 (5 µM) for 10 min. Cell division did not start to any significant degree during the experiments. Cell migration was studied over a 4-h period under a Nikon (Melville, NY) Diaphot inverted microscope with a x20 phase-contrast objective in an attached, hermetically sealed Plexiglas Nikon NP-2 incubator at 37°C (5). Cell migration was recorded using a JVC (Tokyo, Japan) 1-CCD video camera. Image analysis was performed with a MicroImage analysis system (Cast Imaging, Venice, Italy) and an IBM-compatible system equipped with a video card (Targa 2000; True Vision, Santa Clara, CA). Image analysis was performed by digital saving of images at 15-min intervals. Migration tracks were generated by marking the position of nucleus of individual cells on each image. The net migratory speed (straight-line velocity) was calculated by the MicroImage software based on the straight-line distance between the starting and ending points divided by the time of observation (5). Migration of at least 30 cells was analyzed for each experimental condition. Values are given as means ± SD.

In vitro tube formation

In vitro formation of tubular structures (32) and interaction between HUVEC and SMC were studied on growth factor-reduced Matrigel diluted 1/1 in ice with cold DMEM. To evaluate the endothelial-tube formation, HUVEC were washed twice with PBS, detached with 1% trypsin, and seeded (5 x 104 cells/well) onto Matrigel-coated wells in DMEM containing 0.25% BSA. Cells were periodically observed with a Nikon inverted microscope, and experimental results were recorded at different times. Image analysis was performed with the MicroImage analysis system (Cast Imaging). To investigate the in vitro interaction between endothelial cells and SMC, HUVEC (1 x 106 cells) were labeled with the green fluorescent cell linker PKH2 (2 µM), and SMC (1 x 106 cells) were labeled overnight with the red fluorescent cell linker PKH26 (2 µM) according to the instructions of the manufacturer (Sigma-Aldrich). Cells maintained the fluorescence staining for several days (33). Fluorescent HUVEC were detached, washed, and seeded (5 x 104 cells/well) onto Matrigel-coated wells. HUVEC were then allowed to form spontaneous tubes by overnight incubation in DMEM containing 5% FBS, washed three times with PBS, and cultured with DMEM plus 0.25% BSA. SMC (1.5 x 104 cells/well), stained with red fluorescent PKH26 dye, were detached, washed, and then added to the spontaneously formed endothelial tubes, in the presence of vehicle alone or of sCD154 (100 ng/ml; plus 1 µg/ml enhancer). After 2 h of incubation, the number of SMC associated with endothelial tubes was counted. Pretreatment of SMC with PAF-R antagonist, WEB2170 (5 µM), 10 min before the addition to the formed endothelial tubes, was performed to evaluate whether PAF synthesized by activated endothelial cells mediated HUVEC-SMC interaction.

Cell proliferation assay

Cells were seeded at 10,000 cells/well into 24-well plates in DMEM containing 10% FCS and allowed to adhere. After starvation for 24 h, cells were incubated with different stimuli. After 24- or 48-h incubation, monolayers were carefully washed, dried, and treated with 0.75% crystal violet in a solution of 50% ethanol, 0.25% NaCl, and 1.75% formaldehyde. After washings, the dye was eluted with 1% SDS in PBS, and the absorbance was read at 595 nm with an ELISA reader. Cell number was determined on the basis of a standard curve obtained with known cell numbers of triplicate samples. All experiments were performed in triplicate.

Cell viability assays

Cell viability, in different experimental conditions, was evaluated by the sodium 3'-[1-(phenylaminocarbonyl)-3,4-tetrazolium]-bis(4-methoxy-6-nitro)benzene sulfonic acid hydrate (XTT)-based assay and by the lactate dehydrogenase (LDH) release assay. Cells were cultured in 96-well flat-bottom microtiter plates (Falcon Labware, Oxnard, CA) at a concentration of 5 x 104 cells/well. Cell were appropriately stimulated and, at different periods of time, washed and incubated in serum-free DMEM containing 250 µg/ml XTT at 37°C. XTT reduction was monitored by determination of the absorption values at 620 nm in an automated ELISA reader. LDH activity was measured in the cell-free supernatant using the cytotoxicity detection kit (Roche Diagnostics, Indianapolis, IN) and expressed as percentage of Triton X-100 cell lysate.

Murine angiogenesis assay

Female C57 mice were used at 6–8 wk of age. Angiogenesis was assayed as growth of blood vessels from s.c. tissue into a solid gel of basement membrane Matrigel, containing the test sample (34). Matrigel (8.13 mg/ml), in liquid form at 4°C, was mixed with 40 µg/ml agonist rat anti-mouse CD40 (5), or 100 ng/ml sCD154, and injected (0.5 ml) into the abdominal s.c. tissue of mice, along the peritoneal midline. For inhibition studies, in a selected experimental group, a PAF-R antagonist, WEB2170, was added to the Matrigel (5 µM) and to the drinking water (3 mg/kg/day), and was injected s.c. every day (10 mg/kg), for 4 days consecutively. bFGF (10 ng/ml) was used as positive control. At day 7, mice were killed, and gels were recovered and processed for histology. The tissue was fixed in 10% buffered formalin and embedded in paraffin. Sections cut at 3 µm and stained with H&E were studied by light microscopy. Vessel area and the total Matrigel area were planimetrically assessed from stained sections, as described by Kibbey et al. (35). Only those structures possessing a patent lumen and containing RBC were considered vessels (5). Results were expressed as percentage ± SE of the vessel area to the total Matrigel area.

Statistics

Nonparametric statistical analysis was performed by the Kruskal-Wallis test for ANOVA followed by Dunnett’s test for comparison of groups vs one control, and by the Newman-Keuls test for comparison among pairs of groups.


   Results
Top
 Abstract
 Introduction
 Materials and Methods
 Results
Discussion
 References
 
CD40 activation stimulated PAF synthesis by HUVEC but not SMC

Fig. 1 shows the results of experiments performed to investigate whether CD154 induced synthesis of PAF by endothelial cells. The rate of PAF synthesis was determined both by bioassay on washed rabbit platelet aggregation (Fig. 1A) and by incorporation of the [3H]acetate precursor in the PAF molecule (B). Whereas unstimulated HUVEC produce only a minimal amount of PAF, stimulation with sCD154 induced significant PAF synthesis. PAF was also produced by HUVEC incubated with 1 x 106 J558L, a murine plasmocytoma stably expressing CD154, but not with the empty transfectant J558 used as control. PAF synthesized by HUVEC after stimulation with sCD154 remained mainly cell associated, because it was undetectable in cell-free supernatants (data not shown). Fig. 1C shows the time course of PAF synthesis by HUVEC after stimulation with sCD154, J558L, and thrombin. PAF synthesis peaked 5 min after stimulation to decrease thereafter. Whereas the synthesis of PAF by thrombin and J558L was transient, the one obtained after stimulation with sCD154 was higher and was sustained up to 60 min.



View larger version (10K):
[in this window]
[in a new window]
  		FIGURE 1. PAF synthesis by HUVEC (1 x 106 cells) stimulated for 5 min at 37°C with 100 ng/ml sCD154 (plus 1 µg/ml enhancer), or coincubated with 1 x 106 of J558 cells transfected to express CD154 (J558L), or with the empty vector (J558), or stimulated with 1 U/ml thrombin (THR) used as control. A, PAF extracted from cells was determined after TLC purification by a bioassay of washed rabbit platelet aggregation. ANOVA with Dunnett’s multicomparison test was performed between vehicle vs treatment (*, p < 0.05). B, PAF extracted from cells was determined by incorporation of the [3H]acetate precursor in the PAF molecule (see Material and Methods). Data represent means ± SD of three individual experiments. ANOVA with Dunnett’s multicomparison test was performed between vehicle vs treatment (*, p < 0.05). C, Time course of PAF synthesis by HUVEC (1 x 106 cells) stimulated with 100 ng/ml sCD154 (plus 1 µg/ml enhancer), with 1 U/ml thrombin (THR) or with 1 x 106 of J558L or J558. PAF was detected as cell associated. Data are the means ± SD of three individual experiments.

 
Because platelets are known to express CD154 after thrombin activation (30), the synthesis of PAF was also studied after incubation of HUVEC with human platelets expressing CD154 upon preincubation with thrombin. Fig. 2A shows the platelet expression of CD154 after 5 min of treatment with 0.2 U/ml thrombin. Platelets, after inhibition of thrombin with 2 U/ml hirudin (30), were incubated with HUVEC. The effective inactivation of thrombin by hirudin was evaluated on washed rabbit platelet aggregation (not shown). Thrombin-activated platelets induced a significant synthesis of PAF by HUVEC (Fig. 2B) with respect to not-activated platelets. The amount of PAF synthesized after stimulation with activated platelets was higher than that synthesized by J558L and comparable with that obtained by HUVEC stimulation with thrombin. The platelet-free supernatant obtained from platelets treated with thrombin and hirudin did not stimulate PAF synthesis, indicating an effective thrombin inhibition. sCD40-muIg fusion protein inhibited the synthesis of PAF induced by thrombin-activated platelets, indicating that sCD40 prevented the interaction between CD154 expressed by platelets and CD40 expressed by HUVEC (Fig. 2B). The time course of PAF synthesis by HUVEC stimulated with CD154-expressing platelets showed a peak at 5 min followed by a sustained synthesis up to 60 min (Fig. 2C).



View larger version (13K):
[in this window]
[in a new window]
  		FIGURE 2. PAF synthesis by HUVEC stimulated with not-activated or thrombin-activated human platelets. A, Cytofluorimetric analysis of CD154 expression on not-activated (dotted curve) and on 0.2 U/ml thrombin-activated (open curve) human platelets. Figure is representative of three individual experiments. In each experiment, the Kolmogorov-Smirnov statistical analysis between anti-CD154 IgG2a mAb and the isotypic control (solid curve) or between thrombin-treated or untreated human platelets was significant (p < 0.05). B, HUVEC (1 x 106 cells) were incubated with 1.5 x 108 human platelets treated or not with recombinant human thrombin (0.2 U/ml) after thrombin inactivation with 2 U/ml hirudin. To inhibit the CD154-dependent PAF synthesis, HUVEC were stimulated in the presence of 20 ng/ml CD40-muIg fusion protein (CD40-FP). ANOVA with Newman-Keuls multicomparison test was performed among vehicle vs treatment (*, p < 0.05) and among activated platelets vs nonactivated platelets or platelets and CD40-FP (§, p < 0.05). C, Time course of PAF synthesis by HUVEC stimulated with thrombin-activated or not-activated platelets. Data are the means ± SD of four individual experiments.

 
The synthesis of PAF by SMC stimulated with sCD154 was also studied. By cytofluorimetric analysis, SMC expressed an amount of CD40 comparable with HUVEC (data not shown). However, SMC did not synthesize a significant amount of PAF after stimulation of CD40 (unstimulated SMC, 15 ± 2.5 pg per 1 x 106 cells; sCD154-stimulated SMC, 17 ± 3.5 pg per 1 x 106 cells).

Intracellular mechanisms of sCD154-induced PAF synthesis

To determine the intracellular pathway by which CD40 activation induced PAF synthesis in endothelial cells, we pretreated HUVEC with a range of selective inhibitors and investigated their effect on sCD154-induced PAF synthesis. Pretreatment of HUVEC with the specific inhibitor of PLC{gamma} (U73122) and protein kinase C (PKC) (staurosporine and bisindolylmaleimide) and of p38 MAPK (SB203580) induced a significant inhibition of sCD154-induced PAF synthesis (Fig. 3A). As shown in Fig. 3B, sCD154 stimulation of HUVEC induced phosphorylation of PKC{gamma} and of p42/44 MAPK, indicating the activation of the cascade involving PLC{gamma}, PKC, Raf, MAPK kinase, and p42/44 MAPK (36). Indeed, the inhibitory effect on PAF synthesis of U73122 was associated with inhibition of phosphorylation of PKC{gamma} and p42/44 MAPK. The phosphorylation of p42/44 MAPK was also inhibited by bisindolylmaleimide, an inhibitor of PKC. In addition, the involvement of a second cascade implicating p38 MAPK was indicated by phosphorylation of p38 MAPK induced by sCD154 and by the inhibition of PAF synthesis by SB203580 (Fig. 3, A and B). We recently found that CD40 stimulation activates the phosphatidylinositol 3-kinase (PI3K)/Akt-dependent survival pathway (37). We therefore tested the effect of two different inhibitors of PI3K, LY294002 and wortmannin, on PAF synthesis induced by sCD154. We did not find any significant effect of PI3K inhibitors on PAF synthesis (Fig. 3A). Moreover, 4-bromodiphenacylbromide and EDTA, which inhibit the activation of cPLA2, which is involved in the phospholipid remodeling pathway of PAF synthesis, also inhibited the production of PAF (Fig. 3A). As shown in Fig. 3C, sCD154 was able to activate the cPLA2, which is downstream to the activation of both p42/44 MAPK and p38 MAPK pathways, as indicated by the inhibitory effect of bisindolylmaleimide, U73122, and SB203580. Trypan blue exclusion and LDH release experiments indicate that, in similar conditions, the inhibitors used had no toxic effect on HUVEC (data not shown).



View larger version (18K):
[in this window]
[in a new window]
  		FIGURE 3. Effect of selective inhibitors on PAF synthesis, protein phosphorylation, and cPLA2 activation. A, PAF synthesis induced by HUVEC (1 x 106 cells) stimulated for 5 min at 37°C with 100 ng/ml sCD154 (plus 1 µg/ml enhancer) alone or after preincubation for 10 min at 37°C with 10 mM EDTA or specific inhibitor of PKC (100 nM staurosporine and 50 µM bisindolylmaleimide), of PLC{gamma} (10 µM U73122), of PLA2 (1 µM 4-bromodiphenacylbromide), of p38 MAPK (10 µM SB203580), or of PI3K (10 µM LY294002 or 0.1 µM wortmannin). Data represent means ± SD of three individual experiments. ANOVA with Dunnett’s multicomparison test was performed between sCD154 alone vs treatment with inhibitors (*, p < 0.05). B, Western Blot analysis representative of phosphorylation of PLC{gamma} (p-PLC{gamma}), p44/42 MAPK (p-p44/42 MAPK), and p38 MAPK (p-p38 MAPK) after treatment of HUVEC with sCD154 alone or with specific inhibitors (lane 1, untreated; lane 2, 100 ng/ml sCD154 (plus 1 µg/ml enhancer); lane 3, sCD154 plus 10 mM EDTA, lane 4, sCD154 plus 50 µM bisindolylmaleimide; lane 5, sCD154 plus 10 µM U73122; lane 6, sCD154 plus 10 µM SB203580; and lane 7, sCD154 plus 1 µM 4-bromodiphenacylbromide (see Material and Methods)). Three experiments were performed with similar results. C, cPLA2 activity measured in cell lysates after treatment with sCD154 alone or in the presence of selective inhibitors: 10 mM EDTA; 50 µM bisindolylmaleimide (Bisind.); 10 µM U73122; 10 µM SB203580; and 1 µM 4-bromodiphenacylbromide (4-Br.). Data are representative of mean ± SD of three individual experiments.

 
sCD154-stimulated motility of HUVEC

Cell motility of HUVEC was studied by time-lapse recording migration assay (Figs. 4 and 5). Unstimulated cells were first measured and found to remain steady for the whole period of observation never exceeding 10 µm/h. sCD154 significantly enhanced HUVEC migration (Figs. 4B and 5A). Migration started at 15 min and remained sustained for the whole period of observation (Fig. 5B). To investigate the role of PAF, we incubated the cells with two different PAF receptor antagonists, WEB2170 and CV3988, both of which significantly reduced the endothelial motility induced by sCD154 (Figs. 4C and 5), suggesting that PAF mediates, at least in part, the motogenic effect of sCD154. Cell viability, evaluated by an XTT-based assay, was 96 ± 3% on vehicle-treated cells, 96 ± 4.7% on WEB2170-treated cells, and 95 ± 4.3% on CV3988-treated cells. Moreover, the release of LDH in different cell conditions was always <1%.



View larger version (68K):
[in this window]
[in a new window]
  		FIGURE 4. Micrographs representative of time-lapse analysis of HUVEC motility performed by digital saving at 15-min intervals. Migration tracks (magnification, x120) were generated by marking the position of nucleus of individual cells in each image (see Materials and Methods). A, HUVEC stimulated for 4 h at 37°C with vehicle alone. B, HUVEC stimulated with sCD154 (100 ng/ml; plus 1 µg/ml enhancer). C, HUVEC stimulated with sCD154 in the presence of WEB2170 (3 µM).

 


View larger version (17K):
[in this window]
[in a new window]
  		FIGURE 5. Effect of PAF receptor antagonists on sCD154-induced motility of HUVEC. A, Motility of HUVEC stimulated for 4 h at 37°C with sCD154 (100 ng/ml; plus 1 µg/ml enhancer) or PAF (10 ng/ml) in the presence or absence of WEB2170 (3 µM) or CV3988 (5 µM). Motility was monitored by time-lapse analysis and measured as described in Material and Methods. Results are expressed as means ± SD of three individual experiments. ANOVA with Newman-Keuls multicomparison test was performed for sCD154 or PAF vs control (*, p < 0.05); sCD154 vs sCD154 plus WEB-2170 and sCD154 plus CV3988 or PAF vs PAF plus WEB-2170 and PAF plus CV3988 (**, p < 0.05). B, Time course of HUVEC motility induced by sCD154 in the presence or absence of WEB2170 (3 µM). Results are expressed as means ± SD of three individual experiments. ANOVA with Dunnett’s multicomparison test was performed for sCD154 vs sCD154 plus WEB-2170 (*, p < 0.05).

 
sCD154 stimulated in vitro formation of vessel-like structures and interaction between HUVEC and SMC

As shown in Figs. 6, A and B, and 7A, sCD154 stimulated the organization of HUVEC plated on Matrigel with the formation of vessel-like tubular structures. PAF-R antagonist WEB2170 reduced tube formation triggered by stimulation of endothelial CD40 (Figs. 6C and 7A). We also evaluated whether in vitro interaction between endothelial cells and SMC was triggered by PAF synthesized by HUVEC after activation of the CD40/CD154 pathway. HUVEC, stained with green fluorescent PKH2 dye, were allowed to spontaneously form tubes by overnight incubation, and then SMC, stained with red fluorescent PKH26 dye, were added in the presence of vehicle alone or sCD154. After 2 h of incubation, the number of SMC associated with endothelial tubes was counted. As shown in Figs. 6, D and E, and 7B, sCD154 enhanced the interaction between HUVEC and SMC. Pretreatment of SMC with the PAF-R antagonist, WEB2170, before the addition to endothelial tubes, inhibited the interaction between HUVEC and SMC (Figs. 6F and 7B). This result suggests that PAF synthesized by HUVEC mediates, at least in part, their interaction with SMC. Treatment with WEB2170 reduced tube formation below the levels seen with vehicle alone as well as the basal interaction between HUVEC and SMC (Fig. 7). This was not due to a toxic effect of PAF-R antagonists, because vitality, evaluated by the XTT method, was >95%. Indeed, basal proliferation of HUVEC, which is not influenced by PAF (14) was unaffected by WEB2170 (untreated HUVEC, 8,118 ± 11,017; 10 nM PAF-treated cells, 7,950 ± 1,213; 3 µM WEB2170, 7,920 ± 952; 10 nM PAF plus 3 µM WEB2170, 8,010 ± 1,012). A possible explanation is that the basal production of PAF contributes to the spontaneous tube formation and to the basal interaction with SMC. Once the tubes were formed, the addition of WEB2170 to HUVEC did not disrupt the tube network (data not shown).



View larger version (85K):
[in this window]
[in a new window]
  		FIGURE 6. Micrographs representative of in vitro formation of vessel-like structures by HUVEC and interaction between HUVEC and SMC. Tube formation by HUVEC (5 x 104 cells) plated on growth factor-reduced Matrigel (see Materials and Methods) was evaluated after stimulation for 5 h at 37°C with vehicle alone (A), sCD154 (100 ng/ml; plus 1 µg/ml enhancer) (B), or sCD154 (100 ng/ml; plus 1 µg/ml enhancer) in the presence of 3 µM WEB2170 (C). The interaction between HUVEC and SMC was evaluated using HUVEC labeled with green fluorescent cell linker PKH2 plated overnight on Matrigel. After spontaneous tube formation, SMC (1.5 x 104 cells), labeled with red fluorescent cell linker PKH26, were added in the presence of vehicle alone (D) or sCD154 (E). F, SMC were pretreated for 10 min with WEB2170 (3 µM) and then added to HUVEC in the presence of sCD154. Magnification, x120.

 


View larger version (19K):
[in this window]
[in a new window]
  		FIGURE 7. In vitro formation of vessel-like structures by HUVEC and interaction between HUVEC and SMC. A, Tube formation by HUVEC (5 x 104 cells) plated on growth factor-reduced Matrigel was evaluated after stimulation for 5, 12, and 72 h at 37°C with vehicle alone, sCD154 (100 ng/ml; plus 1 µg/ml enhancer), or sCD154 plus 3 µM WEB2170. Data are expressed as the mean ± SD of the tube surface evaluated by the computer analysis system in arbitrary units (a.u.) in five different fields at x20 magnification in duplicate wells of two different experiments. ANOVA with Newman-Keuls multicomparison test was performed between sCD154 vs vehicle (*, p < 0.05); sCD154 plus WEB2170 vs sCD154 or vehicle plus WEB2170 vs sCD154 (**, p < 0.05). B, Percentage of SMC (1.5 x 104 cells labeled with red fluorescent cell linker PKH26) associated to HUVEC (labeled with green fluorescent cell linker PKH2) after 2-h incubation. SMC were added to HUVEC after spontaneous overnight tube formation on Matrigel and after stimulation of HUVEC with vehicle alone (HUVEC alone) or sCD154 (HUVEC sCD154). Where indicated, SMC were pretreated (10 min) with 3 µM WEB2170 (SMC WEB2170) before addition to HUVEC. Data are the means ± SD of four individual experiments. ANOVA with Newman-Keuls multicomparison test was performed for sCD154 vs control (*, p < 0.05); sCD154 plus WEB2170 vs sCD154 or HUVEC alone plus SMC WEB2170 vs HUVEC alone plus SMC alone (**, p < 0.05).

 
Role of PAF on the in vivo neoangiogenesis induced by CD40 stimulation

The in vivo angiogenic effect of CD40 engagement and the potential role of PAF were studied in the murine model of Matrigel s.c. implantation. CD40 engagement induced neoangiogenesis (Fig. 8B) with respect to controls (A). Fig. 8D shows the morphometric analysis of neoangiogenesis induced both by the agonist rat anti-CD40 mAb and sCD154 within Matrigel, 7 days after implantation. PAF-R antagonist WEB2170 inhibited development of neoformed vessels, suggesting that PAF synthesized during the neoangiogenic process contributes to CD40-induced vessel formation (Fig. 8, C and D).



View larger version (73K):
[in this window]
[in a new window]
  		FIGURE 8. Angiogenic effect of CD40 stimulation in vivo. Growth factor-reduced Matrigel (0.5 ml) was mixed with vehicle alone, or with 40 µg/ml agonist rat anti-mouse CD40 mAb (5 ), or with sCD154 (100 ng/ml; plus 1 µg/ml enhancer) or with 40 µg/ml agonist rat anti-mouse CD40 mAb plus 3 µM WEB2170 and injected s.c. in four mice for each experimental group. In the inhibition experimental group, WEB2170 was also added to the drinking water (3 mg/kg/day), and was injected s.c. every day (10 mg/kg), for 4 days consecutively. After 7 days, the mice were killed, and the Matrigel plugs were excised and processed for light microscopy. A, Micrograph representative of control injected with Matrigel and vehicle. B, Micrograph representative of mice injected with Matrigel containing agonist rat anti-mouse CD40 mAb. C, Micrograph representative of mice injected with Matrigel containing agonist rat anti-mouse CD40 mAb plus WEB2170. SC, s.c. tissue. D, Quantification of neoformed vessels was performed on H&E-stained histological sections as described in Materials and Methods, and the results were expressed as the percent mean ± SE of the vessel area to the total Matrigel area.

 

   Discussion
Top
 Abstract
 Introduction
 Materials and Methods
 Results
 Discussion
References
 
The results of the present study indicate that the activation of CD40 induced the synthesis of PAF by endothelial cells. In vitro, it was found that PAF synthesized by HUVEC after stimulation with the CD40 ligand, CD154, is instrumental in the migration and vessel-like organization of endothelial cells, and in the interaction between endothelial cells and SMC. In vivo, blockade of PAF-R prevented the angiogenic effect triggered by CD40 stimulation.

Among the molecular mechanisms that link the immunity to the inflammation, the CD40-CD154 interaction has rapidly emerged as a potential key system, particularly involved in vascular disease processes. In physiological conditions, CD40 is expressed at low levels on endothelial cells, but it is up-regulated in areas of inflammation (8, 38, 39). Recently, CD154 has also been found to be expressed by endothelial cells as well as by SMC, platelets, and macrophages within the atherosclerotic plaque (1).

CD40 stimulation on endothelial cells plays an important role in the phenotypic modulation of the endothelium to an activated state. CD40 was shown to induce expression of proteinases such as collagenase and stromelysin on human monocytes/macrophages, and of collagenase, stromelysin, gelatinase B, and activated gelatinase A on vascular smooth muscle and endothelial cells that may induce plaque destabilization (1, 11, 40). It has been recently shown that inhibition of CD40 signaling limits evolution of established atherosclerosis in mice (9, 10). Ligation of endothelial CD40 by CD154, either expressed on activated monocytes or T cells, or disgorged from platelet granules after activation, stimulated the production of various inflammatory cytokines by endothelial cells (1, 41, 42, 43, 44). Activated platelets, in particular, may have a role in vascular injury, because CD154, which is cryptic in unstimulated platelets, is rapidly expressed on the surface after activation. This may allow the interaction of platelets with endothelial cells via the CD154-CD40 system. Moreover, the surface-expressed CD154 is rapidly cleaved with generation of a soluble CD154, which remains trimeric and biologically active (45). In addition, a soluble form of CD154 released from the surface of tumor cells (13) may contribute to endothelial activation in tumor angiogenesis. We recently found that stimulation of endothelial CD40 triggers neoangiogenesis in vivo, and that its inhibition limits neoangiogenesis and allows apoptotic regression in an experimental model of tumor neoangiogenesis (5).

In the present study, we demonstrate that both sCD154 and membrane CD154 expressed by leukocytes (J558L) or by activated platelets, trigger the synthesis of PAF, a phospholipid mediator of inflammation (17, 18). The amount of PAF synthesized after incubation with J558L was considerably lower than that obtained after incubation with activated platelets. This may depend on the ratio of membrane surface and exposed CD154 per cell and by the number of stimulating cells. The amount of PAF synthesized by HUVEC after stimulation with activated platelets was comparable with that of thrombin, which is considered one of the more efficient stimuli for PAF synthesis by endothelial cells. Therefore, activated platelets are the best candidates for stimulation of PAF synthesis by endothelial cells in vascular injury. Indeed, activated platelets have been suggested as one of the main effector cells in CD40 stimulation in several pathological conditions (45). In endothelial cells, PAF synthesis is known to be mediated via a remodeling pathway in which membrane phospholipids are converted by a PLA2 into lyso-PAF, which is then acetylated by the acetyl-CoA:lyso-PAF acetyltransferase to form PAF (17, 18). It has been recently found that, in bovine aortic endothelial cells, the mechanism of VEGF-induced PAF synthesis involves two intracellular signaling pathways leading to PLA2 activation: a PLC{gamma}-PKC-Raf-p42/p44 MAPK and a MAPK kinase-3/6-dependent activation of p38 MAPK (36). In the present study, we found, using specific inhibitors, that sCD154-induced PAF synthesis by HUVEC depended on both of these pathways. We recently found that CD40 stimulation on endothelial cells activated the PI3K/Akt survival pathway (37). Because it was reported that PI3K plays a negative regulatory role in VEGF-induced PAF synthesis, we tested the effect of two different inhibitors of PI3K, LY294002 and wortmannin. However, we did not observe an enhancement of PAF synthesis after PI3K blockade followed by sCD40 stimulation.

PAF was previously shown to contribute to the angiogenic properties of several polypeptide mediators including VEGF (16). The role of PAF in this contest is possibly mainly related to its motogenic properties that are instrumental in the coordinate migration and in the interaction between endothelial cells required for the formation of new vessels (14, 15, 16). In the present study, we demonstrate that PAF synthesized after stimulation of endothelial CD40 contributed to the in vitro migration and organization of endothelial cells in vessel-like structures and to the in vivo angiogenesis in a murine model of s.c. Matrigel implantation. PAF has been implicated in several inflammatory processes involving angiogenesis, including atherosclerosis (46, 47). In the present study, we provide the first evidence that PAF may be synthesized after engagement of CD40, which has been recently suggested a key signaling pathway in atherosclerosis (2, 3). The synthesis of PAF within the atherosclerotic plaque may amplify the vascular injury by recruiting inflammatory cells and stimulating neoangiogenesis, which may contribute to plaque instability. In addition, we found that PAF also mediated the interaction between endothelial cells organized in tubes and SMC. In these experimental settings, we found that PAF-R blockade inhibited the incorporation of SMC within the endothelial tubes. SMC were unable to synthesize PAF after CD40 stimulation. However, SMC were found to express PAF-R (48, 49) and to proliferate after PAF stimulation (50). The observation that PAF-R antagonism prevented the incorporation of SMC within the endothelial tubes suggests that PAF synthesized by endothelial cells acts on the recruitment of SMC.

In conclusion, these observations provide further evidence for a role of CD40/CD154 in vascular remodeling during inflammation and link this property to the synthesis of PAF by endothelial cells.


   Footnotes
 
1 This work was supported by the Associazione Italiana per la Ricerca sul Cancro, by Italian Ministry of University and Research COFIN 01 and ex60% and FIRB project (RBNE01HRS5-001), by Istituto Superiore di Sanità (Targeted Project AIDS), by Italian Ministry of Health (Ricerca Finalizzata 02), by the National Research Council (Targeted Project Biotechnology), and by the Special Project Oncology, Compagnia San Paolo/FIRMS. Back

2 Address correspondence and reprint requests to Dr. Giovanni Camussi, Cattedra di Nefrologia, Dipartimento di Medicina Interna, Ospedale Maggiore San Giovanni Battista, Corso Dogliotti 14, 10126, Torino, Italy. E-mail address: giovanni.camussi{at}unito.it Back

3 Abbreviations used in this paper: SMC, smooth muscle cell; PAF, platelet-activating factor; VEGF, vascular endothelial growth factor; bFGF, basic fibroblast growth factor; muIg, murine Ig; MAPK, mitogen-activated protein kinase; PL, phospholipase; s, soluble; XTT, 3'-[1-(phenylaminocarbonyl)-3,4-tetrazolium]-bis(4-methoxy-6-nitro)benzene sulfonic acid hydrate; LDH, lactate dehydrogenase; PI3K, phosphatidylinositol 3-kinase; PKC, protein kinase C. Back

Received for publication January 10, 2003. Accepted for publication August 21, 2003.


   References
Top
 Abstract
 Introduction
 Materials and Methods
 Results
 Discussion
 References
 

  1. Mach, F., U. Schonbeck, G. K. Sukhova, T. Bourcier, J. Y. Bonnefoy, J. S. Pober, P. Libby. 1997. Functional CD40 ligand is expressed on human vascular endothelial cells, smooth muscle cells, and macrophages: implications for CD40-CD40 ligand signaling in atherosclerosis. Proc. Natl. Acad. Sci. USA 94:1931.[Abstract/Free Full Text]
  2. Schonbeck, U., P. Libby. 2001. CD40 signalling and plaque instability. Circ. Res. 89:1092.[Abstract/Free Full Text]
  3. Lutgens, E., M. J. Daemen. 2002. CD40-CD40L interactions in atherosclerosis. Trends Cardiovasc. Med. 12:27.[Medline]
  4. Kluth, B., S. Hess, H. Engelmann, S. Schafnitzel, G. Riethmuller, H. E. Feucht. 1997. Endothelial expression of CD40 in renal cell carcinoma. Cancer Res. 57:891.[Abstract/Free Full Text]
  5. Biancone, L., V. Cantaluppi, M. Boccellino, L. Del Sorbo, S. Russo, A. Albini, I. Stamenkovic, G. Camussi. 1999. Activation of CD40 favours the growth and vascularization of Kaposi’s sarcoma. J. Immunol. 163:6201.[Abstract/Free Full Text]
  6. Schonbeck, U., P. Libby. 2001. The CD40/CD154 receptor/ligand dyad. Cell. Mol. Life Sci. 58:4.[Medline]
  7. Grewal, I. S., R. A. Flavell. 1998. CD40 and CD154 in cell-mediated immunity. Annu. Rev. Immunol. 16:111.[Medline]
  8. Reul, R. M., J. C. Fang, M. D. Denton, C. Geehan, C. Long, R. N. Mitchell, P. Ganz, D. M. Briscoe. 1997. CD40 and CD40 ligand (CD154) are coexpressed on microvessels in vivo in human cardiac allograft rejection. Transplantation 64:1765.[Medline]
  9. Schonbeck, U., G. K. Sukhova, K. Shimizu, P. Libby. 2000. Inhibition of CD40 signaling limits evolution of established atherosclerosis in mice. Proc. Natl. Acad. Sci. USA 97:7458.[Abstract/Free Full Text]
  10. Mach, F., U. Schonbeck, G. K. Sukhova, E. Atkinson, P. Libby. 1998. Reduction of atherosclerosis in mice by inhibition of CD40 signalling. Nature 394:200.[Medline]
  11. Mach, F., U. Schonbeck, R. P. Fabunmi, C. Murphy, E. Atkinson, J. Y. Bonnefoy, P. Graber, P. Libby. 1999. T lymphocytes induce endothelial cell matrix metalloproteinase expression by a CD40L-dependent mechanism: implications for tubule formation. Am. J. Pathol. 154:229.[Abstract/Free Full Text]
  12. Melter, M., M. E. J. Reinders, M. Sho, S. Pal, C. Geehan, M. D. Denton, D. Mukhopadhyay, D. Briscoe. 2000. Ligation of CD40 induces the expression of vascular endothelial growth factor by endothelial cells and monocytes and promotes angiogenesis in vivo. Blood 96:3801.[Abstract/Free Full Text]
  13. Bussolati, B., S. Russo, I. Deambrosis, V. Cantaluppi, A. Volpe, U. Ferrando, G. Camussi. 2002. Expression of CD154 on renal cell carcinomas and effect on cell proliferation, motility and platelet-activating factor synthesis. Int. J. Cancer 100:654.[Medline]
  14. Camussi, G., G. Montrucchio, E. Lupia, A. De Martino, L. Perona, M. Arese, A. Vercellone, A. Toniolo, F. Bussolino. 1995. Platelet-activating factor directly stimulates in vitro migration of endothelial cells and promotes in vivo angiogenesis by a heparin-dependent mechanism. J. Immunol. 154:6492.[Abstract]
  15. Montrucchio, G., E. Lupia, E. Battaglia, G. Passerini, F. Bussolino, G. Emanuelli, G. Camussi. 1994. Tumor necrosis factor-{alpha}-induced angiogenesis depends on in situ platelet-activating factor biosynthesis. J. Exp. Med. 180:377.[Abstract/Free Full Text]
  16. Montrucchio, G., E. Lupia, E. Battaglia, L. Del Sorbo, M. Boccellino, L. Biancone, G. Emanuelli, G. Camussi. 2000. Platelet-activating factor enhances VEGF-induced endothelial cell motility and neo-angiogenesis in a murine matrigel model. Arterioscler. Thomb. Vasc. Biol. 20:80.[Abstract/Free Full Text]
  17. Prescott, S. M., G. A. Zimmerman, D. M. Stafforini, T. M. McIntyre. 2000. Platelet-activating factor and related lipid mediators. Annu. Rev. Biochem. 69:419.[Medline]
  18. Pinckard, R. N., D. S. Woodard, H. J. Showell, M. J. Conklyn, M. J. Novak, L. M. McManus. 1994. Structural and (patho)physiological diversity of PAF. Clin. Rev. Allergy 12:329.[Medline]
  19. Ye, R. D., E. R. Prossnitz, A. H. Zou, C. G. Cochrane. 1991. Characterization of a human cDNA that encodes a functional receptor for platelet activating factor. Biochem. Biophys. Res. Commun. 180:105.[Medline]
  20. Honda, Z., M. Nakamura, I. Miki, M. Minami, T. Watanabe, Y. Seyama, H. Okado, H. Toh, K. Ito, T. Miyamoto, T. Shimizu. 1991. Cloning by functional expression of platelet-activating factor receptor from guinea-pig lung. Nature 349:342.[Medline]
  21. Chao, W., M. S. Olson. 1993. Platelet-activating factor: receptors and signal transduction. Biochem. J. 292:617.
  22. Izumi, T., Z. Honda, H. Mutoh, K. Kume, T. Shimizu. 1995. Regulation and signal transduction of PAF receptor. Adv. Prostaglandin Thromboxane Leukotriene Res. 23:461.[Medline]
  23. Saunders, R. N., D. A. Handley. 1987. Platelet-activating factor antagonists. Annu. Rev. Pharmacol. Toxicol. 27:237.[Medline]
  24. P. J. Barnes, and C. P. Page, and P. Henson, eds. Platelet-Activating Factor and Human Disease 1989 Blackwell Scientific, London.
  25. Terashita, Z., S. Tsushima, S. Yoshioka, H. Namoto, Y. Inada, K. Nishikawa. 1983. CV 3988: a specific antagonist of platelet-activating factor (Paf-acether). Life Sci. 32:1975.[Medline]
  26. Heuer, H. O., J. Casals-Stenzel, G. Muacevic, K. H. Weber. 1990. Pharmacologic activity of bepafant (WEB 2170), a new and selective hetrazepinoic antagonist of platelet-activating factor. J. Pharmacol. Exp. Ther. 255:962.[Abstract/Free Full Text]
  27. Camussi, G., M. Aglietta, F. Malavasi, C. Tetta, W. Piacibello, F. Sanavio, F. Bussolino. 1983. The release of platelet-activating factor from human endothelial cells in culture. J. Immunol. 131:2397.[Abstract]
  28. Fridell, Y-W. C., J. Villa, E. C. Attar, E. T. Liu. 1998. GAS6 induces Axl-mediated chemotaxis of vascular smooth muscle cells. J. Biol. Chem. 273:7123.[Abstract/Free Full Text]
  29. Sozzoni, S., P. Allavena, G. D’Amico, W. Luini, G. Bianchi, M. Kataura, T. Imai, O. Yoshie, R. Bonecchi, A. Mantovani. 1998. Differential regulation of chemokine receptors during dendritic cell maturation: a model for their trafficking properties. J. Immunol. 161:1083.[Abstract/Free Full Text]
  30. Urbich, C., Z. Mallat, A. Tedgui, M. Clauss, A. M. Zeiher, S. Dimmeler. 2001. Upregulation of TRAF-3 by shear stress blocks CD40-mediated endothelial activation. J. Clin. Invest. 108:1451.[Medline]
  31. Bligh, E. G., W. J. Dyer. 1959. A rapid method of total lipid extraction and purification. Can. J. Biochem. Physiol. 37:911.
  32. Montesano, R., J. V. Soriano, M. S. Pepper, L. Orci. 1997. Induction of epithelial branching tubulogenesis in vitro. J. Cell. Physiol. 173:152.[Medline]
  33. Horan, P. K., S. E. Slezak. 1989. Stable cell membrane labelling. Nature 340:167.[Medline]
  34. Passaniti, A., R. M. Taylor, R. Pili, Y. Guo, P. V. Long, J. A. Haney, R. R. Pauly, D. S. Grant, G. R. Martin. 1992. A simple, quantitative method for assessing angiogenesis and antiangiogenic agents using reconstituted basement membrane, heparin, and fibroblast growth factor. Lab. Invest. 67:519.[Medline]
  35. Kibbey, M. C., D. S. Grant, H. K. Klieinman. 1992. Role of the SIKVAV site of laminin in promotion of angiogenesis and tumor growth: an in vivo Matrigel model. J. Natl. Cancer Inst. 84:1633.[Abstract/Free Full Text]
  36. Bernatchez, P. N., B. G. Allen, D. S. Gelinas, G. Guillemette, M. G. Sirois. 2001. Regulation of VEGF-induced endothelial cell PAF synthesis: role of p42/44 MAPK, p38 MAPK and PI3K pathways. Br. J. Pharmacol. 134:1253.[Medline]
  37. Deregibus, M. C., S. Buttiglieri, S. Russo, B. Bussolati, G. Camussi. 2003. CD40-dependent activation of phosphatidylinositol 3-kinase/Akt pathway mediates endothelial cell survival and in vitro angiogenesis. J. Biol. Chem. 278:18008.[Abstract/Free Full Text]
  38. Karmann, K., C. C. Hughes, J. Schechner, W. C. Fanslow, J. S. Pober. 1995. CD40 on human endothelial cells: inducibility by cytokines and functional regulation of adhesion molecule expression. Proc. Natl. Acad. Sci. USA 92:4342.[Abstract/Free Full Text]
  39. Biancone, L., G. Segoloni, E. Turello, D. Donati, B. Bussolati, G. Piccoli, G. Camussi. 1998. Expression of inducible lymphocyte costimulatory molecules in human renal allograft. Nephrol. Dial. Transplant. 13:716.[Abstract/Free Full Text]
  40. Schonbeck, U., F. Mach, G. K. Sukhova, C. Murphy, J. Y. Bonnefoy, R. P. Fabunmi, P. Libby. 1997. Regulation of matrix metalloproteinase expression in human vascular smooth muscle cells by T lymphocytes: a role for CD40 signaling in plaque rupture?. Circ. Res. 81:448.[Abstract/Free Full Text]
  41. Thienel, U., J. Loike, M. J. Yellin. 1999. CD154 (CD40L) induces human endothelial cell chemokine production and migration of leukocyte subsets. Cell. Immunol. 198:87.[Medline]
  42. Slupsky, J. R., M. Kalbas, A. Willuweit, V. Henn, R. A. Kroczek, G. Muller-Berghaus. 1998. Activated platelets induce tissue factor expression on human umbilical vein endothelial cells by ligation of CD40. Thromb. Haemostasis 80:1008.[Medline]
  43. Dechanet, J., C. Grosset, J. L. Taupin, P. Merville, J. Banchereau, J. Ripoche, J. F. Moreau. 1997. CD40 ligand stimulates proinflammatory cytokine production by human endothelial cells. J. Immunol. 159:5640.[Abstract]
  44. Schonbeck, U., F. Mach, J. Y. Bonnefoy, H. Loppnow, H. D. Flad, P. Libby. 1997. Ligation of CD40 activates interleukin 1{beta}-converting enzyme (caspase-1) activity in vascular smooth muscle and endothelial cells and promotes elaboration of active interleukin 1{beta}. J. Biol. Chem. 272:19569.[Abstract/Free Full Text]
  45. Henn, V., J. R. Slupsky, M. Grafe, I. Anagnostopoulos, R. Forster, G. Muller-Berghaus, R. A. Kroczek. 1998. CD40 ligand on activated platelets triggers an inflammatory reaction of endothelial cells. Nature 391:591.[Medline]
  46. Subbanagounder, G., N. Leitinger, P. T. Shih, K. F. Faull, J. A. Berliner. 1999. Evidence that phospholipid oxidation and/or platelet activating factor play an important role in early atherogenesis: in vitro and in vivo inhibition by WEB 2086. Circ. Res. 85:311.[Abstract/Free Full Text]
  47. Brochériou, I., D. Stengel, L. Mattsson-Hultén, J. Stankova, M. Rola-Pleszczynski, F. Koskas, O. Wiklund, Y. Le Charpentier, E. Ninio. 2000. Expression of platelet-activating factor receptor in human carotid atherosclerotic plaques: relevance to progression of atherosclerosis. Circulation 102:2569.[Abstract/Free Full Text]
  48. Chaqour, B., P. S. Howard, C. F. Richards, E. J. Macarak. 1999. Mechanical stretch induces platelet-activating factor receptor gene expression through the NF-{kappa}B transcription factor. J. Mol. Cell. Cardiol. 31:1345.[Medline]
  49. Jeanneton, O., M. Delvaux, A. Botella, J. Frexinos, L. Bueno. 1993. Platelet-activating factor (PAF) induces a contraction of isolated smooth muscle cells from guinea pig ileum: intracellular pathway involved. J. Pharmacol. Exp. Ther. 267:31.[Abstract/Free Full Text]
  50. Cirillo, P., P. Golino, M. Ragni, C. Battaglia, F. Pacifico, S. Formisano, C. Buono, M. Condorelli, M. Chiariello. 1999. Activated platelets and leucocytes cooperatively stimulate smooth muscle cell proliferation and proto-oncogene expression via release of soluble growth factors. Cardiovasc. Res. 43:210.[Abstract/Free Full Text]



This article has been cited by other articles:


Home page
 Clin. Cancer Res.Home page
S. Doublier, M. Ceretto, E. Lupia, S. Bravo, B. Bussolati, and G. Camussi
The Proangiogenic Phenotype of Tumor-Derived Endothelial Cells is Reverted by the Overexpression of Platelet-Activating Factor Acetylhydrolase
Clin. Cancer Res., October 1, 2007; 13(19): 5710 - 5718.
[Abstract] [Full Text] [PDF]

Home page
 J. Exp. Med.Home page
C. Chiodoni, M. Iezzi, C. Guiducci, S. Sangaletti, I. Alessandrini, C. Ratti, F. Tiboni, P. Musiani, D. N. Granger, and M. P. Colombo
Triggering CD40 on endothelial cells contributes to tumor growth
J. Exp. Med., October 30, 2006; 203(11): 2441 - 2450.
[Abstract] [Full Text] [PDF]

Home page
 Arterioscler. Thromb. Vasc. Bio.Home page
R. Virmani, F. D. Kolodgie, A. P. Burke, A. V. Finn, H. K. Gold, T. N. Tulenko, S. P. Wrenn, and J. Narula
Atherosclerotic Plaque Progression and Vulnerability to Rupture: Angiogenesis as a Source of Intraplaque Hemorrhage
Arterioscler. Thromb. Vasc. Biol., October 1, 2005; 25(10): 2054 - 2061.
[Abstract] [Full Text] [PDF]

This Article
Right arrow Abstract Freely available
Right arrow Full Text (PDF)
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Right arrow Citation Map
Services
Right arrow Similar articles in this journal
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Citing Articles
Right arrow Citing Articles via HighWire
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by Russo, S.
Right arrow Articles by Camussi, G.