Laboratory for Skeletal Disorders and Rehabilitation, Department of Orthopedic Surgery, Children’s Hospital, Harvard Medical School, Longwood Avenue, Boston, Massachusetts; and
* Department of Cancer Immunology & AIDS, Dana-Farber Cancer Institute, and Departments of
Medicine and
Pathology, Harvard Medical School, Binney Street, Boston, Massachusetts
 TOP ABSTRACT INTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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Key Words: integrins • delayed-type hypersensitivity • CD44 • metalloproteases
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TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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Osteopontin has been implicated in cell attachment [10
11
12
] and cell motility [13
, 14
]. The protein binds to two types of receptors. Engagement of the homing receptor CD44 through a non-RGD cell-binding domain of osteopontin is sufficient to induce chemotaxis or attachment [14
, 15
]. Binding osteopontin to 
vß3 integrin receptors via its Gly-Arg-Gly-Asp-Ser (GRGDS) motif [12
, 16
, 17
] may contribute to osteoclast adherence and resorption of bone [18
] as well as to haptotaxis of endothelial cells [19
], vascular smooth muscle cells [17
, 20
], myelomonocytic cells [21
], and tumor cells [22
]. Vascular smooth muscle cells may also engage osteopontin through vß1 and vß5 integrins in an interaction that leads to adhesion of cells but not to migration [13
], and adhesion to immobilized osteopontin via integrins 4 and 5 has been reported [21
]. Engagement of integrin 9ß1 may induce migration [23
]. Osteopontin is secreted in nonphosphorylated [24
25
26
27
] and phosphorylated forms [28
29
30
], which contain up to 28 phosphate residues and are differentially induced by tumor promoters and cytokines. Phosphorylation is functionally important, as it may determine whether osteopontin associates with the cell surface or with the extracellular matrix [31
, 32
]. Furthermore, cleavage of osteopontin with thrombin may enhance its cell attachment properties [33
]. These results suggest that osteopontin may elicit specific cellular responses depending on its post-translational modification and the cell surface receptor repertoire on its target cell.
The structural basis for the interaction of osteopontin with macrophages leading to migration and perhaps activation is incompletely understood, as earlier studies have often equated function with cell adherence. Prior experiments were performed mostly with cells of different lineages, and it has been shown for other extracellular matrix proteins, including thrombospondin and fibronectin, that their interactions with macrophages could not be predicted from such studies. The necessity for cell attachment of the RGD motif in recombinant osteopontin has been confirmed in mutational analysis. Mutagenesis of the RGD sequence to RAA completely abrogated the interaction of melanoma cells with osteopontin, and mutagenesis of the RGD to RGE resulted in 50% reduction in the attachment of these cells to osteopontin [23 ]. Mutagenizing the RGD to RGE in mouse osteopontin eliminated the attachment of tumor cells and gingival fibroblasts [34 ]. Analyses of further structural requirements for osteopontin functions have also demonstrated that phosphorylation may be essential for integrin-mediated cell adhesion [32 ] and may confer attachment of osteoclasts. It has not been clear whether additional sequences are necessary for osteopontin interaction with its integrin receptors and whether such sequences determine a second binding site or steric modifiers that expose the RGD sequence after phosphorylation. The role of osteopontin phosphorylation in other functions has not been investigated. We have recently found phosphorylation to be essential for various cytokine functions of osteopontin [35 36 37 ]. Here, we show that engagement of ß3-integrin and CD44 receptors by separate domains of osteopontin leads to the expression of distinct macrophage-response phenotypes, which can be separated on the level of biological function, and that the interaction of integrin receptors with osteopontin is regulated by phosphorylation of specific sites on the ligand. We examine macrophages as the cell type that is physiologically predominantly affected by osteopontin, and we compare native osteopontin to recombinant protein that has been phosphorylated on specific sites.
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TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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vß3-, CD44- murine embryonic fibroblast clone derived from BALB/c 3T3 cells (CCL-163, ATCC). A31 cells transfected with CD44 (A31.C1) or A31 mock transfectants were generated as described [14
].
Osteopontin purification and cleavage
Recombinant mouse glutathione-S-transferase-osteopontin fusion protein was derived from Escherichia coli, digested with factor Xa and purified by affinity chromatography, as described [40
, 41
]. Osteopontin was purified to homogeneity as determined by N-terminal sequencing. The native osteopontin used in this study was isolated from bone cell cultures or from MC3T3E1 cells and is a full-length protein that is O-glycosylated and highly sialylated, free of sulfate or N-glycosylation, and contains 15–17 phosphate residues. Thrombin cleavage and phosphorylation of the dephosphorylated, native protein or recombinant osteopontin were accomplished by human thrombin (Sigma Chemical Co., St. Louis, MO), protein kinase A, protein kinase G, Golgi kinases, or purified casein kinase II or casein kinase I as described [12
, 29
, 30
, 40
41
42
]. Dephosphorylation was performed using type II potato acid phosphatase [35
]. Endotoxin levels of purified osteopontin were below 1 ng/g according to Limulus lysate analysis [35
].
In preliminary experiments, MH-S cells attached to but did not spread on phosphorylated and unphosphorylated PNGRGDSLAYGLR synthetic peptides. Therefore, we attempted to isolate a proteolytic fragment that can promote cell spreading. Partial tryptic, chymotryptic, and Asp-N endopeptidase digestion of osteopontin did not result in the isolation of an active peptide; however, a 10-kD fragment was isolated from a Lys-C digest that mediated the spreading of macrophages at approximately 40% (mol/mol) of the activity of the N-terminal thrombin fragment. The N-terminal sequence of this peptide was determined to be QETLPSN. Based on size and sequence analysis of this peptide, referred to as NT10k, we predict that it terminates at the thrombin cleavage site. It contains seven potential phosphorylation sites and approximately 5 mol phosphate/mol peptide. Upon dephosphorylation of this peptide, spreading activity is lost but can be regained by rephosphorylation with Golgi kinases.
Chemotaxis
Directed migration of cells was determined in multiwell chemotaxis chambers [14
, 43
]. Two-well culture plates (transwell) with polycarbonate filters (pore size 8–12 µm) separating top and bottom wells were coated with 5 µg fibronectin. Cells (2x105) were added to the upper chamber and incubated at 37°C in the presence or absence of osteopontin in the lower chamber. After 4 h, the filters were removed, fixed in methanol, and stained with hematoxylin and eosin, and cells that had migrated to various areas of the lower surface were counted microscopically. Controls for chemokinesis included 200 ng of the appropriate form of osteopontin in the top well. For inhibition studies, the cells were incubated with the relevant antibodies for 15 min before adding to the upper well of the transwell chamber. All assays were done in triplicates and are reported as mean ± standard error.
Haptotaxis
Haptotaxis of monocytic cell lines to osteopontin or fragments of osteopontin was assayed using a Boyden chamber. The lower surface or both sides of polycarbonate filters with 8 µm pore size were coated with the indicated amounts of osteopontin. Cells (2x105) were added to the upper chamber and incubated at 37°C in the absence of any factors in the lower chamber. After 4 h, the filters were removed, fixed in methanol, and stained with hematoxylin and eosin. Cells that had migrated to the lower surface were counted under a microscope. All assays were done in triplicates and are reported as mean ± standard error.
In vivo cell migration
Female C57BL/6 mice, purchased from Jackson Laboratories (Bar Harbor, MA) and housed at the Redstone Animal Facility of the Dana-Farber Cancer Institute (Boston, MA), were injected intraperitoneally (i.p.) with 200 µl phosphate-buffered saline (PBS) containing varying dosages of K7 osteosarcoma-derived osteopontin. Injections of vehicle alone (PBS) served as negative controls. The mice were sacrificed by CO2 asphyxiation at varying times after injection followed by immediate collection of peritoneal exsudate by i.p. injection and recovery of twice 10 mL PBS. Red blood cells were removed by hypotonic lysis with ACK buffer (0.15 M NH4Cl, 1.0 mM KHCO3, 0.1 mM Na2 EDTA, pH 7.4) for 5 min at room temperature. Cells were washed and resuspended in Dulbecco’s modified Eagle’s medium containing 5% fetal bovine serum for fluorescent antibody staining at a concentration of 0.2–1 million cells in 50 µl. Fluorescence-labeled antibodies (1 µg/1x106 cells) were incubated with cells for 30 min at 4°C, before washing twice with 200 µl PBS and fixation in 500 µl 2% paraformaldehyde in PBS. Analysis for cellular expression of CD44 (Pgp-1, phycoerythrin) together with CD11b [membrane attach complex (Mac)-1, FITC, macrophage marker], B220 (FITC, B cell marker), or CD3 (FITC, T cell marker) was performed by dual-color flow cytometry with antibodies from PharMingen (San Diego, CA) using a Coulter (Miami, FL) EPICS flow cytometer. Appropriate, nonspecific antibody controls and single-color controls were included.
Cell attachment and spreading
Cell adhesion is a prerequisite for chemotaxis, haptotaxis, and cell spreading. In vitro assays revealed that cells display passive and active adhesion. Active adhesion is pH- and temperature-dependent, reduced by trypsin treatment, and dependent on cell viability. Passive adherence is temperature- and pH-independent, unaffected by trypsin treatment, and independent of cell viability. Maximal levels of active adherence by macrophages depend on harvest of cells without enzymes from subconfluent cultures and limited exposure to temperature fluctuation. In these studies, we distinguish among cell passive adhesion, active adhesion, and spreading. Passive adhesion is not associated with rearrangement of the cytoskeleton: Attached (possibly adhered) cells cannot undergo G0-G1 transition (as judged by cyclin D expression) and become nonviable within 6–12 h. Actively adherent cells rearrange their cytoskeleton, can undergo G0-G1 transition, and proliferate. Spread cells are arrested cells in G2, do not proliferate, and are characterized by focal adhesion plaques. Most dye-binding assays cannot differentiate these different types of attachment. Dye-binding assays, such as crystal violet, which bind very tightly to dead cells, do not allow differentiation between cell debris and live, actively attached cells.
Twenty-four-well plates were coated overnight at 4°C with 10 µg/ml of the indicated ligand and were then blocked for 1 h at room temperature with 10 mg/ml bovine serum albumin (BSA) in PBS. At these concentrations, the osteopontin-derived ligands are several orders of magnitude in excess of the estimated numbers of receptors on the plated cells and are considered saturating so that moderate differences in ligand binding to the plastic do not affect the experiment. To preserve the integrity of adhesion receptors, MH-S monocytic cells were harvested from subconfluent cultures by nonenzymatic cell-dissociation solution (Sigma Chemical Co.). The cells were washed twice with PBS and resuspended at a concentration of 1 x 105 cells/ml in sterile Ca2+- and Mg2+-free PBS supplemented with 0.1% BSA and 1 mM sodium pyruvate. Cells (5x104) were incubated in each well, and after 1 h at 37°C, the wells were washed three times with 0.5 ml PBS to remove nonadherent cells, fixed in 1% glutaraldehyde in 0.1 M cacodylate buffer (pH 7.4) at room temperature for 1 h, and were then stained with toluidine blue and hematoxylin. The total number of attached or spread cells in each well was counted microscopically using a Nikon Eclipse microscope equipped with a Sony digital camera. Total number of attached or spread cells was quantitated using Optima 5.2 image analysis system. Each experiment was done in triplicates and is reported as mean ± standard error. To minimize variability inherent to cell-attachment studies, we scored cells as attached only when a defined nucleus was observed accompanied by a transition from round to cuboidal cell morphology. Round cells are loosely attached with no defined nucleus and were scored as nonattached. These cells can be removed with repeated washes. The viability of the cells was measured before and after the termination of the experiments, and only data from experiments with greater than 95% cell viability were used. Further, under the conditions used in these experiments, cell attachment was temperature-dependent, inhibitable by trypsin treatment, and not affected by inhibitors of protein synthesis or secretion. Cell spreading was determined by membrane-contour analysis and was scored according to increase in cell volume/surface area. In some experiments, cell spreading was also assessed by the formation of stress fibers. Each experiment was performed in quadruplicate wells and repeated three times.
Zymography
Secretion of proteinases was assayed by sodium dodecyl sulfate (SDS)-substrate gel electrophoresis under nonreducing conditions as described [44
, 45
]. Cell culture supernatant was collected after 6 h of culture, concentrated five times, and resuspended in 200 µl zymogram buffer (40 mM Tris, pH 7.5) before addition to Laemmli sample buffer and electrophoresis in 10% polyacrylamide gels, impregnated with 1 mg/ml gelatin. Following electrophoresis, gels were incubated for 30 min at 37°C in 50 ml 50 mM Tris-HCl buffer, pH 8.0, containing 2% Triton X-100 and 10 mM CaCl2 to remove the SDS, followed by incubation for 18 h in 50 mM Tris-HCl buffer, pH 8.0, containing 5 mM CaCl2. After staining the gels with Coomassie brilliant blue, gelatin-degrading enzymes were identified as clear bands against a dark blue background.
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TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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Figure 1. Titration of osteopontin into the peritoneum induces a cellular infiltrate in a dose-dependent manner. The numbers reflect induction ratios after 6 h of (A) total cells ( ) or (B) cells with the surface markers Mac-1+ ( ), B220+ ( ), or CD3+ ( ) in mice injected with osteopontin versus mice injected with PBS (baseline cell numbers for PBS-injected mice ranged from 443,000 to 1.1x106 cells total; 224,000 to 596,000 Mac-1+ cells; 31,300 to 176,000 B220+ cells; 18,100 to 214,100 CD3+ cells). The data points are combined from three experiments. Error bars, where indicated, are mean ± SE.
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The C-terminal domain of osteopontin interacts with CD44 to induce chemotaxis
Earlier studies of osteopontin binding to the myelomonocytic cell line Wehi 3 suggested that this interaction depended mainly on engagement of integrin receptors [16
], and later investigations identified CD44 as a second receptor that was associated with chemotaxis [14
]. As thrombin cleaves osteopontin in two sites releasing two large fragments, an N-terminal 1–153 fragment containing the RGD motif and a 158–294 C-terminal fragment [33
], and as previous studies have demonstrated that the attachment of tumor cells is mediated preferentially by RGD-containing domains of osteopontin [48
], we exploited these observations to determine whether distinct domains of osteopontin were responsible for engagement of the two receptors. The macrophage cell lines MT-2/1 and MH-S express the relevant receptors, integrin ß3 and CD44, at high levels according to flow cytometry. Although one form containing variant exons appears to be the most prominent CD44 gene product as judged by PCR with primers for the constitutive exons 5 and 16, three bands between 200 and 400 base pairs are amplified with primers for exon 5 and exon v6. Expression of standard CD44 was not detected (Fig. 2
).
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Figure 2. Expression of CD44 and integrin ß3 by MH-S and MT-2 cells. The expression levels of CD44 and integrin ß3 were measured by flow cytometry with FITC-conjugated antibodies to these surface receptors (anti-pan-CD44 clone IM7 and 2C9.G2) and an irrelevant control antibody (open peak, not labeled). RT-PCR with primers for the constitutive exons 5 and 16 of CD44 (MT-2 CD44 and MH-S CD44) amplifies a prominent band of about 200 bp in macrophage cell lines (with these primers, the standard form would yield a product of 135 bp; ref. [39
]), indicating that standard CD44 is not abundantly expressed. RT-PCR with primers for the exons 5 and v6 (MT-2 v6 and MH-S v6) results in three PCR products, ranging in size from 200 bp to 400 bp, corroborating the expression of multiple CD44 variants that contain the exon v6. No bands were seen in the no-template controls (H2O CD44 and H2O v6). The two lateral lines indicate the positions of the markers for 194 bp and 300 bp.
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Table 1. Migratory Activity of Osteopontin and Its Thrombin Fragments
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As some osteopontin functions are dependent on the phosphorylation of the ligand, we attempted to localize the critical residues for haptotaxis. Phosphorylation has to occur at specific sites, as Golgi kinases and casein kinase I or II can activate osteopontin, whereas protein kinase A or G phosphorylates the recombinant molecule but does not confer integrin binding (Table 1E) . Earlier studies, which showed that RGD-containing peptides can confer function, may have induced nonspecific effects through multiple integrin receptors. Our data demonstrate that the RGD motif is necessary but not sufficient to confer specific osteopontin function; a sequence N-terminal to the RGD sequence is also needed.
The N-terminal domain of osteopontin induces spreading and activation of macrophages via integrin ß3
Macrophage spreading on extracellular matrix proteins depends, in part, on engagement of their integrin receptors. Spreading of the MH-S macrophage cell line on immobilized, native osteopontin is mediated by the RGD-containing N-terminal thrombin cleavage fragment but not by the C-terminal fragment and is reversed by addition of soluble GRGDS but not control GRGES peptide. Moreover, phosphorylation of recombinant osteopontin is required for this activity (Fig. 3
).
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Figure 3. Phosphorylation of osteopontin is required to induce cell spreading. MH-S monocytic cells (103/well) or MT-2/1 cells (not shown) were incubated in 96-well plates that had been coated with 10 µg/ml (300 nM) indicated ligands for 1 h before washing, staining with toluidine blue, and counting. (Top) Change in cell morphology: MH-S cells attached to and spread on immobilized phosphorylated osteopontin; MH-S cells bound to unphosphorylated osteopontin do not spread (original magnification, 400x). (Middle) Numbers of cells attached to the indicated ligands in the presence or absence of GRGDS peptide or of the control peptides GRGES or SGRSD. Values are expressed as mean ± SE. (Bottom) Numbers of cells spread on the indicated ligands in the presence or absence of GRGDS. Values are expressed as mean ± SE. rOPN, Recombinant osteopontin; -P, native, phosphorylated osteopontin; -, no osteopontin; NT, N-terminal thrombin cleavage fragment of osteopontin; CT, C-terminal fragment.
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(TNF-) but not IL-1ß, IL-10, or IL-6. Additional analysis revealed that cytokine induction depends on the interaction between phosphorylated osteopontin and peritoneal macrophages (Fig. 5
). This interaction was mediated by the N-terminal portion of osteopontin and was inhibited by GRGDS and integrin ß3 antibody (not shown).
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Figure 4. Induction of metalloprotease secretion by phosphorylated but not unphosphorylated osteopontin. MH-S cells were stimulated for 6 h with phosphorylated or unphosphorylated osteopontin at a concentration of 10 µg/ml (300 nM) in serum-free, defined medium. To visualize the secreted metalloproteases, gelatin zymograms were performed. MMP-9 and pre-MMP-9 are visible in the sample stimulated with natural osteopontin (lane 2) and samples stimulated with phosphorylated recombinant osteopontin (lane 3). Dephosphorylation of osteopontin with acid phosphatase abolishes the stimulatory activity of osteopontin (lane 4). Similarly, recombinant osteopontin has no stimulatory activity (lane 5). The pre-form but not active MMP9 is stimulated by the N-terminal fragment of osteopontin (lane 6), and the C-terminal fragment of osteopontin has little or no stimulatory activity (lane 7). Control, MH-S cells were incubated with serum-free, defined medium (lane 1).
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Figure 5. Osteopontin induces secretion of inflammatory mediators from macrophages. Resident peritoneal macrophages, obtained by peritoneal lavage with PBS, were treated with red cell lysis buffer and incubated (105 macrophages per 100 µl) for 2 h. The adherent fraction was incubated with 5 nM osteopontin (OPN, native osteopontin; dpOPN, dephosphorylated native osteopontin; rOPN, recombinant osteopontin; rOPN P, recombinant osteopontin phosphorylated by Golgi kinases) or 30 ng/ml LPS. Supernatant IL-12, TNF-, IL-1ß, IL-10, and IL-6 were assayed at 24 or 48 h post-stimulation with commercial enzyme-linked immunosorbent assay kits (R&D Systems, Minneapolis, MN). Similar results were obtained with the MH-S cell line.
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TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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The participation of monocytes/macrophages in inflammation entails emigration of these cells from peripheral blood into infected tissues, where they produce cytokines that regulate diverse processes including antimicrobial activity, cell growth, differentiation, and wound healing [49
]. Emigration of monocytes depends on coordinate engagement of different subsets of cell surface receptors by cytokines and extracellular matrix that underlie migration or adhesion within various anatomic compartments. Osteopontin plays an important role in macrophage infiltration in response to pathological stimuli [50
]. Our findings suggest that attraction and activation of monocytes depend, in part, on orchestrated activities of osteopontin-binding domains that have been modified by thrombin [22
], ecto-kinases [51
], and ecto-phosphatases [32
]. Thrombin cleavage of osteopontin that has been integrated into the matrix through transglutaminases [52
] can lead to the release of a chemotactic C-terminal osteopontin fragment and attraction of monocytes to a site of infection. Subsequent engagement of integrin receptors on emigrant monocytes by the immobilized, phosphorylated N-terminal domain of osteopontin may facilitate local haptotactic migration toward a site of microbial infection or inflammation (Fig. 6
). After arrival, attachment and spreading of emigrant monocytes mediated by engagement of vß3 integrin receptors by the N-terminal osteopontin thrombin cleavage product (possibly through increased access of the RGD-binding site; ref. [19
]) can lead to macrophage activation and expression of inflammatory mediators such as metalloproteases and cytokines (Fig. 5)
. The cytokine profile reflects a type 1 pattern and in conjunction with the coordinated regulation of macrophage migration and invasion, accounts for the prominent role played by the cytokine osteopontin in cellular immunity [35
]. The coupling of macrophage cell shape and gene expression through the linkage of cytoskeletal networks to the extracellular matrix provides a molecular framework for differential responses to various presentations of the same ligand [53
]. Although additional in vivo studies are required to test this model, the definition of the functional domains of osteopontin in this report represents an important step in understanding this process and may allow the rational development of osteopontin analogs that antagonize or mimic discrete biological activities of the parent molecule.
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Figure 6. Model of monocyte regulation by osteopontin. Osteopontin is secreted by activated T cells. Thrombin cleavage releases the two receptor-binding domains, which carry out distinct functions in the cascade of events leading to macrophage attraction and activation. The C-terminal piece exerts chemotactic activity that is phosphorylation-independent, leading to attraction of macrophages to the cleavage site and cellular attachment to the osteopontin N-terminal fragment. Phosphorylation-dependent haptotaxis on cross-linked osteopontin or OPN-NT leads to macrophage spreading and activation, including induction of cytokine secretion and release of metalloproteases that can degrade the matrix.
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Received January 27, 2002; revised June 5, 2002; accepted June 14, 2002.
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 E. E. Rollo, S. J. Hempson, A. Bansal, E. Tsao, I. Habib, S. R. Rittling, D. T. Denhardt, E. R. Mackow, and R. D. Shaw The Cytokine Osteopontin Modulates the Severity of Rotavirus Diarrhea J. Virol., March 15, 2005; 79(6): 3509 - 3516. [Abstract] [Full Text] [PDF]
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 F. Giacopelli, R. Marciano, A. Pistorio, P. Catarsi, S. Canini, G. Karsenty, and R. Ravazzolo Polymorphisms in the osteopontin promoter affect its transcriptional activity Physiol Genomics, December 15, 2004; 20(1): 87 - 96. [Abstract] [Full Text] [PDF]
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 Z. Xie, M. Singh, and K. Singh Osteopontin Modulates Myocardial Hypertrophy in Response to Chronic Pressure Overload in Mice Hypertension, December 1, 2004; 44(6): 826 - 831. [Abstract] [Full Text] [PDF]
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 M. Gattorno, A. Gregorio, F. Ferlito, V. Gerloni, A. Parafioriti, E. Felici, E. Sala, C. Gambini, P. Picco, and A. Martini Synovial expression of osteopontin correlates with angiogenesis in juvenile idiopathic arthritis Rheumatology, September 1, 2004; 43(9): 1091 - 1096. [Abstract] [Full Text] [PDF]
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 J. S. Berman, D. Serlin, X. Li, G. Whitley, J. Hayes, D. C. Rishikof, D. A. Ricupero, L. Liaw, M. Goetschkes, and A. W. O'Regan Altered bleomycin-induced lung fibrosis in osteopontin-deficient mice Am J Physiol Lung Cell Mol Physiol, June 1, 2004; 286(6): L1311 - L1318. [Abstract] [Full Text] [PDF]
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K. Tanaka, J. Morimoto, S. Kon, C. Kimura, M. Inobe, H. Diao, G. Hirschfeld, J. M. Weiss, and T. Uede Effect of Osteopontin Alleles on {beta}-Glucan-Induced Granuloma Formation in the Mouse Liver Am. J. Pathol., February 1, 2004; 164(2): 567 - 575. [Abstract] [Full Text] [PDF]
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 C. Gao, H. Guo, L. Downey, C. Marroquin, J. Wei, and P. C. Kuo Osteopontin-dependent CD44v6 expression and cell adhesion in HepG2 cells Carcinogenesis, December 1, 2003; 24(12): 1871 - 1878. [Abstract] [Full Text] [PDF]
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D. Leali, P. Dell'Era, H. Stabile, B. Sennino, A. F. Chambers, A. Naldini, S. Sozzani, B. Nico, D. Ribatti, and M. Presta Osteopontin (Eta-1) and Fibroblast Growth Factor-2 Cross-Talk in Angiogenesis J. Immunol., July 15, 2003; 171(2): 1085 - 1093. [Abstract] [Full Text] [PDF]
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E. S. Roberts, M. A. Zandonatti, D. D. Watry, L. J. Madden, S. J. Henriksen, M. A. Taffe, and H. S. Fox Induction of Pathogenic Sets of Genes in Macrophages and Neurons in NeuroAIDS Am. J. Pathol., June 1, 2003; 162(6): 2041 - 2057. [Abstract] [Full Text] [PDF]
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