| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
|
|
|
|||||||
|
|||||||||
Hematologic Diseases Branch, Division of AIDS, STD, and TB Laboratory Research, National Center for Infectious Diseases, Centers for Disease Control and Prevention, Atlanta, GA 30333
 |
Abstract |
|---|
 Top Abstract IntroductionMaterials and MethodsResultsDiscussionReferences |
|---|
|
Introduction |
|---|
|
TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
|---|
production in macrophages (7). The anticoagulant protein C zymogen, when activated by the thrombin/thrombomodulin complex, becomes a serine protease in the natural anticoagulant pathway (8). Classically, APC has functioned not only to inactivate the procoagulant factors Va and VIIIa (9, 10) but to also neutralize the activity of plasminogen-activator inhibitor-1 (PAI-1) (11). Further underscoring the importance of APC as an anticoagulant protein was the recent observation that the molecular basis of resistance to activated protein C or Factor V Leiden was a mutation in an APC cleavage site of Factor V (12, 13).
The protein C/protein S anticoagulant pathway has been suggested to be
a common link between coagulation and inflammation (1). Animal studies
have demonstrated that an infusion of APC could block the lethal
effects of disseminated intravascular coagulation in Escherichia
coli-induced sepsis (14). Data from these studies indicated that
APC may play a role in the inflammatory response by modulating the
effects of cytokines such as TNF and by blocking neutrophil activation
(7, 15, 16). These observations have been supported by more recent in
vitro studies in which it was shown that not only could protein C and
APC block E-selectin-mediated cell adhesion (17) but, as alluded to
earlier, APC has been shown to block LPS, phorbol ester, and
-IFN-induced TNF production (7). In further support of the protein
C/protein S pathway serving as a link between inflammation and
coagulation was the observation that infusion of the APC cofactor,
protein S, reversed the deleterious effects of infused C4bBP in
E. coli-induced sepsis (18).
The production of cytokines has an important role in the pathogenesis of many diseases, particularly those with an inflammatory component. In the inflammatory state, cytokines are part of a host’s response to maintain or restore hemostatic balance. Cytokines can function to induce the acute-phase response, initiate mononuclear cell migration to the site of injury, induce wound repair, and both augment and amplify the immune response. More recent data have implicated cytokines such as IL-8 as important physiologic participants in cross-talk between coagulation and inflammation (19). In addition to being beneficial, cytokines can also have a deleterious effect on the host. Acute and chronic inflammation as well as thrombosis are among the pathologic conditions that have a significant cytokine component (1, 20, 21).
Following vascular injury, there is an exquisite interplay between coagulation, anticoagulation proteins, cytokines, and inflammatory cells in an attempt to resolve injury. Not only is the endothelium fundamental to the resolution of injury through the elaboration of chemotactic cytokines and expression of adhesion molecules that allow the recruitment and adherence of neutrophils, monocytes, and lymphocytes, but it is also pivotal in maintaining a balance between the procoagulant and anticoagulant forces. These multiple interrelated functions are thought to be linked, and, in support of the protein C/protein S anticoagulant pathway serving as one possible common link between inflammation and coagulation, we report that APC can up-regulate the expression of the proinflammatory cytokines IL-6 and IL-8 in endothelial cells.
|
Materials and Methods |
|---|
|
TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
|---|
Purified protein C, protein S, activated protein C, and the chromogenic substrate 2-oxo-4-thiazolidine carboxyl-prolyl-arginyl-paranitroanilide-HCl (TCPA-pNA) for the determination of APC amidolytic activity were obtained from Celsus Laboratories (Cincinnati, OH). Other commercial sources of APC were American Diagnostica (Greenwich, CT), Alexis (San Diego, CA), and Enzyme Research (South Bend, IN). With indicated exceptions, experiments were performed with APC preparations obtained from Celsus Laboratories. Before use, lyophilized activated protein C was rehydrated in sterile distilled water and dialyzed overnight against cold PBS, pH 7.3. Frozen (-70°C) APC (Enzyme Research) was used without dialysis. DFP, Hirudin, E. coli LPS, and polymyxin B were obtained from Sigma, St. Louis, Mo. A purified murine Ab (No. 2375) specific for the epidermal growth factor (EGF)5-EGF6 region of thrombomodulin and capable of inhibiting thrombomodulin-mediated protein C activation and a goat polyclonal (No. 2377) Ab to human thrombomodulin were obtained from American Diagnostica.
Cell culture
HUVEC, human coronary artery endothelial cells (HCAEC), and human microvascular endothelial cells (HMVEC) were obtained from Clonetics (San Diego, CA) and propagated using the manufacturer’s medium MCDB 131 with 5% FCS and accompanying instructions. The HepG2 hepatocellular carcinoma cell line was obtained from the American Type Culture Collection (ATCC, Manassas, VA). HepG2 cells were grown in Eagle’s minimal essential medium and were maintained as previously described (5). Cells, propagated as monolayer cultures, were initially plated at a density of 1 x 105 cells/cm2 in 0.33-cm2 96-well plates (Costar, Chantilly, VA), or for RNA harvest in 75-cm2 culture flasks. Once cells reached confluence, supernatant fluids were removed by aspiration, and fresh complete media with or without added protein C, protein S, or APC was added to the cell monolayers. Cell viability was determined by a neutral red uptake assay followed by absorbance measurement at 570 nm as described previously (22). Culture supernatant fluids were harvested at the indicated time-points and either used immediately in ELISA determinations or frozen at -70°C for later analysis.
ELISA
Commercial kits were obtained and used for the measurement of IL-6 (R&D Systems, Minneapolis, MN, and CYTImmune Science, College Park, MD) and IL-8 (Biosource International, Camarillo, CA) according to the manufacturer’s protocols. Absorbance was determined with an EL312e Microplate Reader (Biotek, Winooski, VT) and data reduction was accomplished with the KinetiCalc software package (Biotek).
APC chromogenic assay
APC (0.04 nmol/ml) was preincubated with 5 U hirudin at room temperature for 30 min before addition to 2.5 µmol/ml TCPA-pNA substrate in a final volume of 100 µl of 1% BSA-PBS, pH 8.2, in 96-well clusters (Costar). The change in optical density at 405 nm was monitored at 1-min intervals with an EL312e kinetic plate reader (BioTek).
APC inactivation by DFP
DFP treatment of APC was conducted at room temperature for 2 h at a final concentration of 2 µM and followed by overnight dialysis against PBS, pH 7.6, at 4°C before addition to the culture media.
Ribonuclease protection assay (RPA)
Total cellular RNA was isolated using a Tri-Reagent isolation
kit (Sigma) according to the manufacturer’s protocol. RPAs were
performed using RiboQuant (PharMingen, San Diego, CA) also according to
the manufacturer’s instructions. Two RiboQuant kits were used. The
hCK-2 contained probes for human IL-12p35, IL-12p40, IL-10, IL-1,
IL-1ß, IL-1Ra, IL-6, IFN-, ribosomal L32, and
glyceraldehyde-3-phosphate dehydrogenase (GAPDH), while the hCK-5 set
contained Ltn (lymphotoxin), RANTES, IP-10, MIP-1ß, MIP-1,
monocyte chemoattractant protein (MCP)-1, IL-8, L32, and GAPDH.
The probes L32 and GADPH were provided in each kit to ensure that
equivalent amounts of RNA were present in each lane. Briefly, labeled
riboprobes ([32P]UTP) were prepared from plasmids
containing probe inserts supplied by the manufacturer. Labeled probes
were hybridized overnight with 15 to 20 µg of RNA, and the reactions
were subsequently digested with a mixture of RNase A and T1 for 45 min
followed by proteinase K digestion for 15 min. Riboprobe-RNA complexes
were isolated using a phenol-chloroform extraction step and
ethanol-acetate precipitation. The RNA-riboprobe complexes were then
run on an 8-M urea sequencing gel for 2 h at 55°C. After drying,
the gel was exposed to x-ray film from 1 to 5 days.
Electrophoretic mobility shift assay
Radiolabeled probes were made from double-stranded oligonucleotides synthesized according to the sequence of the NF-IL-6 binding site (bp -163 to -139 5'-ACG TCACATTGCACAATCTTAATAA-3'). Nuclear proteins were extracted and prepared as described (23), and 5 µg of protein was incubated with 1x binding buffer, 5% glycerol, 0.1% Nonidet P-40, 1 µg poly(dI-dC) (Bandshift Kit, Pharmacia LKB Biotechnology, Piscataway, NJ), and DNA probes in a final volume of 20 µl. Competitive binding assays contained 30x, 50x, or 100x molar excess unlabeled DNA probe. After 20 min at room temperature, the reaction mixture was analyzed for protein-DNA binding by 6% native polyacrylamide gel electrophoresis in 0.25% Tris-borate-EDTA buffer. Autoradiographs were from gels that were dried and exposed to x-ray film (Hyperfilm-MP, Amersham Life Science, Arlington Heights, IL).
|
Results |
|---|
|
TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
|---|
APC up-regulation of both IL-6 and IL-8 in HUVECs occurred in a
dose-dependent fashion within a range of 0 to 90 nM (Fig. 1
, A and B). At the
equivalent protein C physiologic concentration of 
50 nM, APC had no
effect on either endothelial cell viability or proliferation. However,
APC at 180 nM did elicit a change in cellular morphology and decreased
the viability of endothelial cells (data not shown). As determined by
ELISA, significant increases in both IL-6 and IL-8 production were
detected as early as 8 h after the addition of APC, and cytokine
levels continued to increase through 48 h (Fig. 1, C
and D). These increases in cytokine levels, with increasing
APC concentrations or exposure over time, compared with control levels
(Fig. 1, A–D), were statistically significant by
Student’s t test (range p < 0.001- <
0.05). The effect of APC on endothelial cell IL-6 and IL-8 production
was significantly potentiated (p < 0.01) when
the APC-purified cofactor, protein S, was added to cell cultures in
combination with APC (Fig. 2,
A and B). However, when used alone, neither
purified protein S nor protein C had any effect on IL-6 or IL-8
production (Fig. 2, A and B). On a
transcriptional level, IL-6 RNA was up-regulated by 50 nM APC at 3
h but returned to control levels by 6 h (Fig. 3A), whereas IL-8
up-regulation was observed at 3 h and 6 h and returned to
near control levels by 24 h (Fig. 3B). In some
experiments a modest induction of the p35 chain of IL-12 was observed,
but, unlike IL-6 and IL-8, this effect was not consistent in all
experiments. No induction of either IL-1, IL-1ß, IL-10, IL-1Ra,
-IFN, RANTES, lymphotoxin, IP-10, MIP-1, or MIP-1ß RNA was
observed (data not shown).
|
|
|
The inactivation of APC by DFP demonstrated that the active site
of APC was required for cytokine up-regulation as shown for IL-8 in
Figure 4. APC activity was also inhibited
by the serine protease inhibitor, aprotinin (1 TIU/ml), further
documenting the specificity of APC (Fig. 4). To rule out possible
thrombin or LPS contamination of the APC preparation as a source of
cytokine up-regulation, experiments were conducted using the respective
inhibitors, hirudin and polymyxin B, which alone had no effect on APC
activity. Hirudin, up to concentrations of 20 U/ml, had no effect on
the ability of APC to up-regulate IL-6/IL-8. (Fig. 4). It should be
noted, however, that thrombin alone at 
10 U/ml (5x the amount
that should be expected in the APC preparation based on a typical
protein C activation with EDTA/thrombin (24)) did up-regulate IL-6 and
IL-8, but the effect was completely inhibited by coincubation with
excess hirudin (data not shown). When used alone at 
5 U/ml, thrombin
had no measurable effect on IL-6 or IL-8 production. Similarly,
polymyxin B (10 µg/ml) had no effect on the action of APC (Fig. 4),
thereby indicating that the effect was not due to LPS contamination. In
further support that the effect was not due to LPS, endothelial cell
activation by the APC preparation was heat labile and was abolished
after heating the preparation at 56°C for 30 min (Fig. 4). At the
concentrations employed, neither hirudin, aprotinin, or polymyxin B had
any effect on cell morphology, viability, IL-6, or IL-8 levels. At
concentrations ranging from 50 to 250 nM, purified protein C had no
effect on the APC-mediated up-regulation of either IL-6 or IL-8 (Fig. 2
and Fig. 5). Preincubation of up to
fivefold excess of protein C in cell culture 30 min before the addition
of APC did not diminish or block APC-mediated up-regulation of either
IL-6 or IL-8 (Fig. 5). Furthermore coincubation of APC with threefold
molar excess murine monoclonal anti-thrombomodulin or an eightfold
molar excess immunopurified goat anti-thrombomodulin Abs had no
effect on cytokine up-regulation (data not shown).
|
|
or IL-1ß was not
observed, experiments using IL-1Ra were conducted to further exclude
the possibility that IL-1 may have been responsible for IL-6/IL-8
up-regulation. IL-1Ra at the concentrations of 10 ng/ml had no effect
on APC induction of either IL-6 or IL-8, thereby demonstrating that the
APC effect was IL-1 independent (data not shown).
To establish that the APC effect was not unique to one commercial
preparation, purified APC was obtained from three other commercial
sources. As illustrated in Table I, each
APC preparation had the ability to significantly increase the
production of IL-6/IL-8 from endothelial cells over that of basal
levels. APC from Enzyme Research Laboratories had the greatest effect
with approximately a 44- and 18-fold increase in IL-6 and IL-8
production, respectively. The potency of the APC preparation from
Enzyme Research was further highlighted by its high amidolytic
(functional) activity as compared with the other commercial sources
(Table I).
|
Since it has been reported that IL-6 could up-regulate the vitamin
K-dependent anticoagulant protein, protein S, in the HepG-2 cells (25),
experiments were conducted to determine what effect IL-8 may have on
protein S production. As shown in Figure 6, while having no direct effect itself,
IL-8 synergized with IL-6 to significantly increase protein S
production over that of IL-6 alone in the HepG-2 cells. IL-8 had no
effect on protein S production in endothelial cells (data not shown),
which was not surprising, since these cells have no IL-8 receptors
(26).
|
As shown in Figure 7, APC, in a
dose-response fashion, induced IL-6 and IL-8 in both the microvascular
and coronary artery endothelial cells (Fig. 7, A-D). As
depicted in Figure 8, microvascular
endothelial cells produced 2 to 3 times more IL-6 and IL-8 in response
to 50 nM of APC than did HUVECs. Coronary artery endothelial cells
produced significantly less IL-6 and IL-8 than HUVECs, in response to
APC, and 3 to 4 times less IL-6 and IL-8 than did the microvascular
endothelial cells (Fig. 8). Furthermore, compared with both HUVECs and
microvascular endothelial cells, APC at the concentration of 50 nM
induced only a modest increase in IL-6 and IL-8 production in coronary
artery endothelial cell (CAEC) cultures. The experimental data
sets for Figures 7 and 8 were generated with APC obtained from Enzyme
Research Labs, hence the overall greater levels of IL-6/IL-8 induction
compared with Figures 1, 2, 4, and 5.
|
|
The transcriptional factor NF-IL-6 was maximally expressed at 30
min with a decrease in expression noted at 60 min following exposure to
50 nM APC (Fig. 9). Specificity of the
response was determined by using unlabeled DNA as a competitive
inhibitor at a 30-fold and 100-fold excess.
|
|
Discussion |
|---|
|
TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
|---|
Though the anticoagulant role of APC is well recognized, little is known about its effect in the acute but localized inflammatory state that involves the microvasculature. This report provides data that suggest that APC, in addition to its anticoagulant properties, may also function to restore hemostasis via cytokine induction. The finding that APC significantly increased the production of both cytokines, particularly IL-8, in the microvascular endothelial cells, as compared with the HUVECs and the coronary artery endothelial cells, was especially interesting since leukocyte trafficking and the development of the inflammatory response occurs in the microvasculature. Moreover, the observation that endothelial cells from coronary arteries produced the least amount of IL-6/IL-8 in response to APC was not surprising since it could be argued that a robust inflammatory response in this particular vascular bed probably would not be advantageous to the host.
Our data, together with work by Johnson et al. (19), which reported an increase in IL-8 production during coagulation, suggest the following. Concomitant with limiting clot formation, APC could induce IL-8 production independent of coagulation to produce enough IL-8/IL-6 to achieve one of two opposing physiologic endpoints, with the outcome dependent on the extent of injury. One endpoint would be the maintenance of IL-8/IL-6 levels required to maintain leukocyte trafficking and adherence at the site of injury, thereby amplifying the inflammatory response. In addition, increased levels of both IL-6 and IL-8 could also contribute to the restoration of the integrity of the endothelium by formation of a fibrin clot by inducing thrombogenesis through the induction of tissue factor in monocytes (28). Conversely at the other endpoint, the inflammatory response could be attenuated by APC through alterations in the local IL-8 concentration gradient that would inhibit rather than induce neutrophil migration (29, 30), and, likewise, increased IL-6 levels would also contribute to the inhibition of neutrophil accumulation (31). In indirect support of the latter, a recent report demonstrated that APC inhibited LPS-induced pulmonary vascular injury by inhibiting the accumulation of activated neutrophils (16). Furthermore, increased levels of IL-6, mediated by APC, not only would serve to induce the acute phase response but could increase the levels of protein S, the cofactor for APC (32). In addition, the observation that IL-8 could synergize with IL-6 to up-regulate hepatic derived protein S (25) within a specific time-frame further suggests that APC may be able to control its enzymatic activity via the indirect up-regulation of protein S. Our data does in fact demonstrate that exogenously added protein S can increase IL6/IL-8 production induced by APC.
Members of the serine protease family, which includes APC, have become recognized as important mediators in leukocyte function (33). Some of the newly recognized functions of serine proteases include induction of apoptosis, chemotaxis, cell adhesion, and proliferation, as well as cytokine modulation. It is thought that these proteases initiate their cellular effects through signal transduction via protease receptors. Factor Xa, a serine protease that has been classically defined as a clotting protein responsible for catalyzing the activation of prothrombin to thrombin, has recently been shown to induce cellular proliferation. Gajduseck et al. (6) have reported that factor Xa induced endothelial cell proliferation through the induction of platelet-derived growth factor. These observations were extended by Gasic et al. (34), in which it was shown that smooth muscle cell proliferation was induced by factor Xa. In contrast to endothelial cells, the effect of factor Xa on smooth muscle cells was independent of any known mitogens or cytokines.
The mechanism(s) through which APC exerted its effect on endothelial
cells is presently not known. However, since DFP blocked the ability of
APC to up-regulate IL-6/IL-8, it was apparent that the APC active site
was necessary for its biologic effect. DFP has been used by many
investigators to block the active site to determine APC specificity.
Grey et al. (7) used DFP to show that APC could block TNF production by
human macrophages, while Hancock et al. (35) used it to demonstrate
that high affinity APC receptors were present on these phagocytic
cells. We have further demonstrated specificity by abolishing the APC
effect through the use of the serine protease inhibitor, aprotinin. In
further support of APC specificity, the APC cofactor, protein S, was
shown to augment IL-6/IL-8 up-regulation when exogenously added
together with APC. Contamination of the APC preparation with thrombin
or LPS was ruled out since inhibitors of both thrombin and LPS failed
to abolish cytokine up-regulation and furthermore neither purified
protein C or protein S, when used alone, had any effect. Although
thrombin was also capable of IL-6 and IL-8 up-regulation, much higher
levels were required (10 U/ml) than would be expected if residual
thrombin were present in the APC preparation.
Since APC up-regulated IL-6/IL-8 at the transcriptional level, which in part may have been due to the induction of the NF-IL-6 transcriptional factor, it could perhaps be argued that the APC effect was receptor mediated. Receptors for APC have been identified on both macrophages (36) and endothelial cells (37, 38). Recent investigations have suggested that the Ca2+-independent macrophage APC receptor is probably distinct from the Ca2+-dependent APC receptor found on endothelial cells. Although our preliminary data suggest that the APC effect is Ca2+ independent (our unpublished observations), we have yet to determine whether or not the effect is mediated through a specific receptor. The observed APC effect was also probably independent of the endothelial cell protein C receptor (EPCR) (37) since protein C not only was unable to induce IL-6/IL-8 but also could not block the effect of APC. The APC effect was also independent of APC-thrombomodulin interaction since anti-thrombomodulin Abs had no effect on IL-6/IL-8 induction by APC. Presently, we cannot rule out the possibility that APC may act through a nonreceptor mechanism by the formation of a complex with protein S on the phospholipid membrane of the endothelial cell or that APC may initiate an intracellular signal via the cleavage of a membrane-bound serine protease-sensitive protein.
In summary it can be argued that our results suggest that, in addition to the benefits reported by others, APC may also have a negative effect on the host through the induction of proinflammatory cytokines. Although this possibility cannot be excluded, we would like to propose that APC may contribute to the resolution of injury in part by regulating cytokine production crucial to the regulation of either the early or delayed inflammatory response, and that the magnitude of this response may be dependent on the type or location of the vascular bed. These results further extend the biologic functions of a protein that has classically been defined as an anticoagulant protein and provides further evidence for a role for APC in the inflammatory response.
|
Acknowledgments |
|---|
|
Footnotes |
|---|
2 Abbreviations used in this paper: APC, activated protein C; DFP, diisopropyl fluorophosphate; HCAEC, human coronary artery endothelial cell; HMVEC, human microvascular endothelial cell; RPA, ribonuclease protection assay; TCPA-pNA, 2-oxo-4-thiazolidine carboxyl-prolyl-arginyl-paranitroanilide-HCl; GAPDH, glyceraldehyde-3-phosphate dehydrogenase; MIP, macrophage inflammatory protein.
Received for publication October 6, 1997. Accepted for publication April 30, 1998.
|
References |
|---|
|
TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
|---|
down-regulates protein S secretion in human microvascular and umbilical vein endothelial cells but not in the HepG-2 hepatoma cell line. Blood. 84:483., or phorbol ester. J. Immunol. 153:3644.
This article has been cited by other articles:
|
|
 |
|
  S. T.B.G. Loubele, C. A. Spek, P. Leenders, R. van Oerle, H. L. Aberson, K. Hamulyak, G. Ferrell, C. T. Esmon, H. M.H. Spronk, and H. ten Cate Activated Protein C Protects Against Myocardial Ischemia/ Reperfusion Injury via Inhibition of Apoptosis and Inflammation Arterioscler. Thromb. Vasc. Biol., July 1, 2009; 29(7): 1087 - 1092. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 L. O. Mosnier, B. V. Zlokovic, and J. H. Griffin The cytoprotective protein C pathway Blood, April 15, 2007; 109(8): 3161 - 3172. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 C. Feistritzer, R. A. Schuepbach, L. O. Mosnier, L. A. Bush, E. Di Cera, J. H. Griffin, and M. Riewald Protective Signaling by Activated Protein C Is Mechanistically Linked to Protein C Activation on Endothelial Cells J. Biol. Chem., July 21, 2006; 281(29): 20077 - 20084. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 M. Miyamoto, M. Tomaki, J. Lotvall, and A. Linden {beta}-Adrenoceptor stimulation and neutrophil accumulation in mouse airways Eur. Respir. J., August 1, 2004; 24(2): 231 - 237. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
A. W. Rijneveld, S. Weijer, S. Florquin, C. T. Esmon, J. C. M. Meijers, P. Speelman, P. H. Reitsma, H. Ten Cate, and T. van der Poll Thrombomodulin mutant mice with a strongly reduced capacity to generate activated protein C have an unaltered pulmonary immune response to respiratory pathogens and lipopolysaccharide Blood, March 1, 2004; 103(5): 1702 - 1709. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
H. Weiler, V. Lindner, B. Kerlin, B. H. Isermann, S. B. Hendrickson, B. C. Cooley, D. A. Meh, M. W. Mosesson, N. W. Shworak, M. J. Post, et al. Characterization of a Mouse Model for Thrombomodulin Deficiency Arterioscler. Thromb. Vasc. Biol., September 1, 2001; 21(9): 1531 - 1537. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 J. B. Sundstrom, L. K. McMullan, C. F. Spiropoulou, W. C. Hooper, A. A. Ansari, C. J. Peters, and P. E. Rollin Hantavirus Infection Induces the Expression of RANTES and IP-10 without Causing Increased Permeability in Human Lung Microvascular Endothelial Cells J. Virol., July 1, 2001; 75(13): 6070 - 6085. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 J. C. Y. Chan, J. G. Ganopolsky, I. Cornelissen, M. A. Suckow, M. J. Sandoval-Cooper, E. C. Brown, F. Noria, D. Gailani, E. D. Rosen, V. A. Ploplis, et al. The Characterization of Mice with a Targeted Combined Deficiency of Protein C and Factor XI Am. J. Pathol., February 1, 2001; 158(2): 469 - 479. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 D. Ricotta, G. Alessandri, C. Pollara, S. Fiorentini, F. Favilli, M. Tosetti, A. Mantovani, M. Grassi, E. Garrafa, L. Dei Cas, et al. Adult human heart microvascular endothelial cells are permissive for non-lytic infection by human cytomegalovirus Cardiovasc Res, February 1, 2001; 49(2): 440 - 448. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 J T Merrill and R G Lahita Sex hormone binding globulins and atherosclerotic risk in systemic lupus Lupus, March 1, 2000; 9(3): 217 - 222. [Abstract] [PDF]
|
|
|
|
|
|
E. de Jonge, P. E. P. Dekkers, A. A. Creasey, C. E. Hack, S. K. Paulson, A. Karim, J. Kesecioglu, M. Levi, S. J. H. van Deventer, and T. van der Poll Tissue factor pathway inhibitor dose-dependently inhibits coagulation activation without influencing the fibrinolytic and cytokine response during human endotoxemia Blood, February 15, 2000; 95(4): 1124 - 1129. [Abstract] [Full Text] [PDF]
|
|
| ||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||
| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
