Search tips
Search criteria 


Logo of jcinvestThe Journal of Clinical Investigation
J Clin Invest. 2002 October 1; 110(7): 923–932.
PMCID: PMC151148

PPARγ ligands inhibit primary tumor growth and metastasis by inhibiting angiogenesis


Several drugs approved for a variety of indications have been shown to exhibit antiangiogenic effects. Our study focuses on the PPARγ ligand rosiglitazone, a compound widely used in the treatment of type 2 diabetes. We demonstrate, for the first time to our knowledge, that PPARγ is highly expressed in tumor endothelium and is activated by rosiglitazone in cultured endothelial cells. Furthermore, we show that rosiglitazone suppresses primary tumor growth and metastasis by both direct and indirect antiangiogenic effects. Rosiglitazone inhibits bovine capillary endothelial cell but not tumor cell proliferation at low doses in vitro and decreases VEGF production by tumor cells. In our in vivo studies, rosiglitazone suppresses angiogenesis in the chick chorioallantoic membrane, in the avascular cornea, and in a variety of primary tumors. These results suggest that PPARγ ligands may be useful in treating angiogenic diseases such as cancer by inhibiting angiogenesis.


PPARγ is a ligand-activated nuclear receptor that is critical in a variety of biological processes, including adipogenesis, glucose metabolism, and inflammation (1). Genetic knockout of PPARγ in mice interferes with terminal differentiation of trophoblasts and vascularization of the placenta, resulting in death by embryonic day 10 (2). PPARγ functions as an important cellular regulator by inhibiting growth and/or inducing differentiation of adipocytes, monocytes, and cancer cells, including those of breast, colon, and liposarcoma (37).

PPARγ is the molecular target of the thiazolidinedione (TZD) class of antidiabetic drugs, which includes rosiglitazone and troglitazone. It has been shown that TZDs suppress the growth of several cancer lines, including colon, breast, and prostate, in vitro and in vivo (6, 8, 9). However, TZDs have minimal to no inhibitory activity on other tumor lines in vitro (5, 8, 10, 11). In fact, high levels of PPARγ in tumor cells do not always correlate with growth inhibition by TZDs in vitro, suggesting that tumor cells can acquire resistance to direct TZD effects (5, 8, 12). Most importantly, TZDs have antitumor effects in PPARγ-deficient embryonic stem cell tumors (12). Together these findings suggested that the antitumor effects of PPARγ ligands may not be mediated entirely through the tumor cell itself.

We hypothesized that the tumor endothelium is a potential target of TZDs, since primary tumor and metastatic growth are dependent on angiogenesis (13). This hypothesis is supported by the observations that PPARγ is expressed in endothelial cells, and that PPARγ ligands can inhibit their proliferation induced by growth factors or cause their apoptosis in vitro (1417). In addition, TZDs inhibit choroidal neovascularization when administered intraocularly (18). Interestingly, there is recent evidence suggesting that PPARγ is localized in tumor endothelial cells (19). However, the role of PPARγ ligands in tumor angiogenesis has not been studied.

Here we report, for the first time to our knowledge, that PPARγ is expressed at high levels in tumor endothelium and can be activated in endothelial cells by its ligands. We show that PPARγ ligands, such as rosiglitazone, inhibit primary tumor growth and metastasis by both direct and indirect antiangiogenic effects. These findings are clinically relevant because rosiglitazone is an orally administered, FDA-approved drug already used by millions for the treatment of type 2 diabetes. Several other angiogenesis inhibitors have also been identified in drugs originally approved for other indications. These include IFN-α (20), thalidomide (21), and celecoxib (22). Results from our studies suggest that PPARγ ligands, such as rosiglitazone, are an addition to this growing class of antiangiogenic drugs for cancer therapy.


Cells and reagents.

Bovine capillary endothelial (BCE) cells were maintained as described (23). Human umbilical vein endothelial cells (HUVECs; VEC Technologies Inc., Rensselaer, New York, USA) were cultured in microvascular endothelial cell growth medium (EGM-2 MV; Clonetics, Walkersville, Maryland, USA). Human glioblastoma cells (U87), prostate carcinoma (LNCaP), T241 fibrosarcoma, human rhabdomyosarcoma cells (RMS559), and Lewis lung carcinoma (LLC) were cultured in DMEM in heat-inactivated 10% FBS. LLC–green fluorescent protein (LLC-GFP) cells were kindly provided by T. Boehm (Children’s Hospital, Boston, Massachusetts, USA). Human liposarcoma tissue specimens were obtained with patient consent and implanted as pieces (1 mm3) subcutaneously into SCID mice (Massachusetts General Hospital, Boston, Massachusetts, USA) in accordance with institutional guidelines of Brigham and Women’s and Children’s Hospitals (Boston, Massachusetts, USA). Tumor was excised under sterile conditions, digested with collagenase and DNase (Roche Diagnostics Corporation, Indianapolis, Indiana, USA), and cultured in DMEM/F-12 media with 20% FBS. Rosiglitazone was kindly provided by GlaxoSmithKline Pharmaceuticals (King of Prussia, Pennsylvania, USA). Troglitazone was kindly provided by Parke-Davis (Ann Arbor, Michigan, USA). WY 14643 was obtained from ChemSyn Laboratories (Lenexa, Kansas, USA).

Preparation of bFGF.

Human bFGF (5′-ATGCCCGCCT TGCCCGAGGA TGGCGGCAGC GGCGCCTTCC CGCCCGGCCA CTTCAAGGAC CCCAAGCGGC TGTACTGCAA AAACGGGGGC TTCTTCCTGC GCATCCACCC CGACGGCCGA GTTGACGGGG TCCGGGAGAA GAGCGACCCT CACATCAAGC TACAACTTCA AGCAGAAGAG AGAGGAGTTG TGTCTATCAA AGGAGTGTGT GCTAA-3′) was expressed in Escherichia coli. The protein was purified by Fast Performance Liquid Chromatography over a HiTrap Heparin column (Amersham Biosciences Corp., Piscataway, New Jersey, USA). The column was washed with 0.8 M NaCl, and bFGF was eluted with 2 M and 3 M NaCl. Fractions containing pure bFGF as determined by silver stain and Western analysis were combined, concentrated, sterilized, and dialyzed into 20 mM sodium citrate, 1 mM EDTA, 9% sucrose, pH 5.0.

Flow cytometry analysis.

A suspension of tumor cells (T241 fibrosarcoma or LLC-GFP) was made by passage of viable tissue through a sieve and treatment with collagenase and DNase. For isolation of skin endothelial cells, murine skin was minced, treated with collagenase and DNase in DMEM, homogenized, and filtered. Cell suspensions were labeled with phycoerythrin-conjugated anti–VEGF receptor-2 and anti–platelet/endothelial cell adhesion molecule (anti-PECAM) antibodies (Pharmingen, San Diego, California). One million positive tumor and skin endothelial cells or GFP-positive LLC cells were collected by FACS.

VEGF, bFGF, and prostatic-specific antigen ELISA.

Tumor cells were plated at 15,000 cells per well (six-well plates) and 24 hours later were treated with rosiglitazone or 0.1% DMSO. Medium containing the drugs was changed on days 3 and 5. Medium was collected on day 6. VEGF and bFGF in the media were assayed by ELISA (R&D Systems Inc., Minneapolis, Minnesota, USA). Serum prostatic-specific antigen (PSA) was measured by ELISA (Beckman Coulter Inc., Fullerton, California, USA) as described (24).

Matrix metalloproteinase and tissue inhibitor of metalloproteinase activity.

Gelatinase activity in the control media and rosiglitazone-treated cells was determined by substrate gel electrophoresis as previously reported (25). Tissue inhibitor of metalloproteinase (TIMP) activity was analyzed using a modified quantitative [14C]collagen film collagenase assay (26).

Western blot analysis.

After 16 hours of treatment, protein was extracted from 60% confluent plates and immunoblotting was performed for PPARγ as described (5). A positive control for PPARγ was obtained from fully differentiated C3H/10T 1/2 cells with adipocyte features, as confirmed with oil red O staining. Total protein extracts (10–30 μg) were analyzed on blots incubated with primary (Calbiochem-Novabiochem Corp., San Diego, California, USA) and secondary antibodies (Amersham Biosciences Corp.). To assay the eIF-2α phosphorylation state after 30 minutes of treatment, protein was extracted from exponentially growing HUVECs and Western blot analysis was performed as described (12).


Surgical specimens of tumors and skin were processed according to standard protocol. Sections were microwaved in 10 mM sodium citrate (pH 6.0) for PPARγ, vWF, MECA-32, and proliferating cell nuclear antigen (PCNA) and were treated with 40 μg/ml proteinase K (Roche Diagnostics Corp.) for 25 minutes at 37°C for PECAM. Mouse anti–human PPARγ (Santa Cruz Biotechnology Inc., Santa Cruz, California, USA), rabbit anti–human vWF (DAKO Corp., Carpinteria, California, USA), rat anti–mouse PECAM (Pharmingen), MECA-32 rat anti–mouse panendothelial cell antigen (Pharmingen), and mouse anti–human PCNA (DAKO Corp.) were incubated at 4°C overnight. PECAM, MECA-32, and PPARγ stainings were amplified using tyramide signal amplification direct and indirect kits (NEN Life Science Products Inc., Boston, Massachusetts, USA). vWF and PCNA were detected with FITC-conjugated secondary antibodies. Rabbit anti-human pericentrin (Covance Inc., Richmond, California, USA) was detected with biotinylated secondary antibody after treatment in ice-cold methanol.

Angiogenesis assays.

Endothelial cell proliferation was assayed as described (23) with 7.5 × 103 cells per well. For tumor cell proliferation, cells were plated at 5 × 103 cells per well. After 24 hours, cells were starved for 12 hours in 0.5% FBS. Cells were treated with TZDs dissolved in 0.1% DMSO. The medium was changed on days 3 and 5. Cells were counted with a particle counter on days 3 and 7.

Chick chorioallantoic membrane (CAM) assays were performed in three separate experiments as described (23). CAMs were observed 48 hours after implantation of a methylcellulose disc (10 μl) with and without rosiglitazone. Corneal neovascularization assays were performed as described (23). After implantation of 80 ng bFGF, TZDs were administered over 6 days by gavage in an aqueous solution of 10% DMSO in 0.5% methylcellulose as described (6), and control mice received vehicle.

For tumor studies, LLC was injected as described (23). Rhabdomyosarcoma and glioblastoma cells were injected subcutaneously (2 × 106 cells in 0.1 ml PBS). Once tumors were 100–200 mm3, mice were randomized into treatment and vehicle groups. TZDs or vehicle were administered by daily gavage for 14–40 days. Tumors were measured every 3–5 days, and volume was calculated as width2 × length × 0.52. Prostate tumor cells (LNCaP) were implanted orthotopically as described (24). Twenty-one days after implantation, mice with serum PSA between 40 and 60 ng/ml were randomized into treatment and vehicle groups. TZDs or vehicle were administered for 17 days (n = 6 mice per group). For metastasis studies, LLC tumors were resected 14 days after implantation as described (23). After LLC resection, mice were treated with TZDs or vehicle for 17 days when control mice became terminally ill. On the last day of treatment, the statistical difference between treatment and control groups was determined by Student’s t test. A P value less than 0.05 was accepted as significant.

Computer-enhanced imaging of tumors.

Histological sections of tumors were analyzed for vessel density by computerized densitometric imaging (Quantimet 570; Leica Inc., Deerfield, Illinois, USA; JVC 3-CCD camera; Victor Co., Tokyo, Japan). The degree of vascularization was quantified over the entire tumor section and expressed as a ratio of vessel area (CD31) to tumor area. Histograms represent the distribution of ratios compiled for 124–314 microscope fields at ×125 magnification.


PPARγ is highly expressed in tumor endothelium in vivo and proliferating endothelial cells in vitro

We first analyzed the expression pattern of PPARγ in the endothelium of normal skin and of various tumors by immunofluorescent double staining for PPARγ and vWF, an endothelial marker. PPARγ was expressed in endothelial and mural cells of normal skin (Figure (Figure1a),1a), in tumor cells, and in the endothelium of all tumors studied including human glioblastoma tissue (Figure (Figure1b).1b). PPARγ localization in the nucleus was confirmed by Hoechst staining.

Figure 1
PPARγ is expressed in endothelium of normal and neoplastic tissues. (a) Immunofluorescent double staining for vWF and PPARγ demonstrates PPARγ expression in endothelium of normal skin. vWF-stained endothelial cells are shown in ...

Although we screened 11 tumor cell lines for a PPARγ-negative tumor, all tumor cell lines expressed PPARγ protein, at varying levels (Figure (Figure1c).1c). To confirm expression of PPARγ in tumor endothelial cells, we separated endothelial cells from a T241 fibrosarcoma cell suspension. Interestingly, PPARγ protein was highly expressed in isolated tumor endothelial cells (Figure (Figure1c).1c). Furthermore, we observed higher expression levels of PPARγ in endothelial cells than in tumor cells when both cell types were isolated from LLC tumors expressing GFP (Figure (Figure1d).1d). In addition, we compared PPARγ expression in proliferating endothelium (tumor) and quiescent endothelium (skin) (Figure (Figure1d).1d). There was a 71% higher expression of PPARγ in tumor endothelium (Figure (Figure11e).

To determine whether endothelial cell growth conditions affect PPARγ expression, we performed immunoblotting on whole-cell lysates of HUVECs under proliferating, contact-inhibited, or starvation conditions. Cells were grown in the presence of 2.5% FBS, bFGF, VEGF, EGF, and IGF-1 in growth-stimulatory conditions and in 0.5% FBS and no growth factors in starvation conditions. In both conditions cells were 60% confluent. We determined that PPARγ protein levels were higher in cells cultured in growth-stimulating conditions compared with those in 6-day 100% confluent cultures (contact-inhibited endothelium) or those in starvation medium (Figure (Figure1f).1f). These data demonstrate that PPARγ expression is higher in proliferating endothelium than in quiescent endothelium.

TZDs induce PPARγ activation in endothelial cells in vitro

Activation of PPARγ by its ligands results in proteolytic degradation of the receptor itself (27). To demonstrate PPARγ activation in endothelial cells, we performed a kinetic study of PPARγ levels in endothelial cells after TZD treatment. After 17 hours of rosiglitazone treatment, PPARγ protein levels decreased in growth factor–stimulated cells in growth media in a dose-dependent manner, indicating PPARγ activation (Figure (Figure2a).2a). Troglitazone similarly reduced PPARγ level in a dose-dependent manner, while PPARα ligand (WY 14643) had no effect. These data demonstrate that PPARγ downregulation results specifically from PPARγ activation (Figure (Figure22b).

Figure 2
TZDs activate endothelial PPARγ in a lactacystin-reversible manner. (a) Western blot analysis of PPARγ protein in proliferating HUVECs. PPARγ protein levels decrease in a dose-dependent manner with rosiglitazone (Rosi). Control, ...

It has been shown that the ubiquitin-proteosome pathway regulates the stability of PPARγ protein in adipocytes (27). Therefore, we asked whether PPARγ is regulated in endothelial cells in a similar manner. In the presence of 2.5 μM lactacystin, a proteosome inhibitor, rosiglitazone failed to trigger PPARγ degradation (Figure (Figure2c).2c). The fact that lactacystin can fully reverse the effect of rosiglitazone suggests that rosiglitazone may induce PPARγ degradation by proteosomes in endothelial cells.

TZDs have direct and indirect antiangiogenic effects in vitro

Direct effects.

To show the effects of endothelial PPARγ activation on cell proliferation, we used BCE cells and induced their proliferation with bFGF, a potent mitogen for BCE cells, in a standard proliferation assay as reported (23, 28, 29). Rosiglitazone inhibited bFGF-induced proliferation of BCE cells in a dose-dependent manner, with maximal inhibition of approximately 94% after a 72-hour incubation period at 1 μM (Figure (Figure3a)3a) and about 69–74% after 7 days of treatment at 0.01–0.1 μM (Figure (Figure3b).3b). Troglitazone had a similar effect on BCE cell proliferation (data not shown).

Figure 3
TZDs have direct and indirect antiangiogenic effects. (a) Percent proliferation of BCE cells is determined by comparing cells exposed to an angiogenic stimulus (bFGF) with those exposed to bFGF and rosiglitazone, relative to unstimulated cells (low serum), ...

In contrast, rosiglitazone did not significantly inhibit proliferation of rhabdomyosarcoma, glioblastoma, LLC, and liposarcoma cells after a 72-hour incubation period, even at doses tenfold (10 μM) the concentration used to inhibit endothelial cells (Figure (Figure3a).3a). Even after 7 days of treatment, rosiglitazone only resulted in maximal inhibition of 26% of liposarcoma and rhabdomyosarcoma cell growth at all concentrations tested, while glioblastoma and LLC were relatively resistant to the antiproliferative effects of rosiglitazone (Figure (Figure3b).3b). Because TZDs activate PPARα and PPARδ receptors at greater than 10 μM (30), we used concentrations of 10 μM and less.

The inhibitory effect of TZDs has recently been suggested to be independent of PPARγ and mediated by inhibition of translation initiation (12). To determine whether endothelial cell growth was inhibited in such a manner, we studied the phosphorylation of translation initiation factor eIF-2α in response to rosiglitazone at the same concentration range as we used for proliferation studies. We found that eIF-2α was partially phosphorylated when HUVECs were treated with 5 μM rosiglitazone and fully phosphorylated with 10 μM rosiglitazone (Figure (Figure3c).3c). However, at 0.01–1 μM rosiglitazone, a concentration that was effective in inhibiting endothelial cell growth, there was no effect on eIF-2α phosphorylation (Figure (Figure3c).3c). These results suggest that the growth inhibitory effect of rosiglitazone on endothelial cells is most likely due to PPARγ activation and not to inhibition of translational initiation.

Indirect effects.

To determine whether rosiglitazone could indirectly inhibit angiogenesis by downregulating tumor-secreted growth factors, we measured bFGF and VEGF levels in tumor-conditioned media. All tumor lines expressed negligible levels of bFGF, but two tumors, glioblastoma and LLC, showed substantial production of VEGF: 20,000 pg/106 cells and 938 pg/106 cells, respectively. Rosiglitazone at 10 μM inhibited VEGF secretion in LLC cells by 56% and at 1 μM inhibited VEGF secretion in U87 cells by 42% (Figure (Figure3d).3d). The inhibitory effect of TZDs on VEGF secretion by tumor cells suggests an indirect effect on the endothelium in vivo via tumor cell production of the angiogenic mitogen VEGF.

PPARγ ligands inhibit CAM angiogenesis and bFGF-induced corneal neovascularization

To test the ability of PPARγ ligands to inhibit in vivo angiogenesis, we examined the effect of rosiglitazone on the de novo growth of blood vessels on the CAMs of 6-day-old chick embryos as reported (23, 28). An advantage of the CAM assay is that it provides a macrophage-free environment until day 8 (31). After 48-hour treatment with rosiglitazone, CAM angiogenesis was inhibited in a dose-dependent manner: 0.1 μg had no effect; 1 μg resulted in a slight inhibitory effect with an avascular zone of 1–2 mm; 2.5 μg caused a 3-mm avascular zone around the disc (Figure (Figure44b).

Figure 4
PPARγ ligands inhibit in vivo angiogenesis in the CAM and bFGF-induced corneal neovascularization. (a) A normal CAM implanted with a methylcellulose disk. (b) After a 48-hour exposure to rosiglitazone (2.5 μg), avascular zones free of ...

To optimize the antiangiogenic doses of TZDs for daily administration in mice, we implanted 80 ng bFGF pellets into the corneas of mice to stimulate corneal neovascularization over 6 days, as reported (23, 28, 29) (Figure (Figure4c).4c). Systemic oral administration of rosiglitazone significantly inhibited angiogenesis in a dose-dependent fashion: 50 mg/kg/d resulted in 39% inhibition (Figure (Figure4d);4d); 100 mg/kg/d, 60% (Figure (Figure4e);4e); 200 mg/kg/d, 61%. Interestingly, much higher doses (400 mg/kg/d) caused only 18% inhibition of vessel growth (Figure (Figure4f).4f). Administration of rosiglitazone twice per day also significantly inhibited angiogenesis at the dose of 5 mg/kg twice a day (36%). Daily administration exhibited a biphasic response with an optimal effect at 100–200 mg/kg/d (Figure (Figure4g).4g). Systemic oral troglitazone also inhibited bFGF-induced corneal angiogenesis (data not shown).

Systemic therapy with PPARγ ligands inhibits a variety of tumors by angiogenesis inhibition

In order to test whether antiangiogenic therapy with PPARγ ligands could suppress the growth of primary tumors, we treated established subcutaneous tumors of 100–200 mm3 volume grown in syngeneic mice as reported (29). Rosiglitazone at 100 mg/kg/d inhibited the growth of glioblastoma, LLC, rhabdomyosarcoma, and liposarcoma by 71%, 60%, 82%, and 69% respectively (Figure (Figure5,5, a–d). There was no evidence of weight loss or other drug-related toxicity in any of the mice. To support our hypothesis that PPARγ ligands can inhibit primary tumor growth by inhibiting angiogenesis, we measured microvessel density in treated and control tumors. A decrease in microvessel density during treatment with an angiogenesis inhibitor suggests that the agent is effective (32). However, because microvessel density has limitations as a surrogate marker for antiangiogenic activity in vivo (33), we also measured endothelial cell proliferation in treated and control tumors.

Figure 5
Systemic therapy with PPARγ ligands inhibits primary tumor growth. After tumors were 100–200 mm3 in size, rosiglitazone treatment (100 mg/kg/d) was initiated (day 0). On the last day of treatment, the statistical difference between control ...

Rosiglitazone treatment reduced vessel density relative to that in the control tumors (Figure (Figure6,6, a–d). In addition, rosiglitazone-treated tumors showed no signs of cytologic differentiation in vivo (Figure (Figure6,6, a–d, insets), while, in vitro, rosiglitazone only induced differentiation of liposarcoma cells (data not shown). By using immunofluorescent double staining for vessels (MECA-32) and proliferation (PCNA), we found a significant decrease in endothelial cell proliferation in rosiglitazone-treated U87 (47%) and LLC (44%) as compared with controls (Figure (Figure66e).

Figure 6
PPARγ ligand therapy reduces vessel density and endothelial cell proliferation. (a, blue inset) Representative control and treated glioblastoma tumors on treatment day 40 are shown. Scale bar, 1 cm. (ad, insets) Hematoxylin-and-eosin ...

To exclude the possibility that the subcutaneous tumor location accounted for sensitivity to antiangiogenic therapy with TZDs, we used an orthotopic human prostate cancer model (24). The prostate cell line (LNCaP) weakly expresses PPARγ, is relatively resistant to TZDs in vitro, and produces PSA (9). We treated established orthotopic prostate tumors with a serum PSA between 40 and 60 ng/ml. After 17 days of treatment with rosiglitazone (100 mg/kg/d) or troglitazone (200 mg/kg/d), PSAs were 73 ± 37 ng/ml or 100 ± 45 ng/ml, respectively, compared with the control group of 235 ± 47 ng/ml. Because TZDs can decrease PSA produced by tumor (LNCaP) cells in vitro with minimal inhibition of tumor cell proliferation (9), we excised tumors to determine whether TZDs had an effect on orthotopic tumor growth. Rosiglitazone- and troglitazone-treated tumors were 72% and 52% smaller by weight than control tumors, respectively. In addition, TZD-treated tumors showed a significant decrease in vessel density (data not shown). Therefore, the antitumor effect of PPARγ ligands can be mediated by antiangiogenesis in both subcutaneous and orthotopic tumor locations.

Systemic therapy with PPARγ ligands prevents metastatic invasion

We next studied the effect of TZDs on tumor metastasis. Mice were treated for 17 days with rosiglitazone (100 mg/kg/d) or vehicle (methylcellulose) after removal of primary LLC. Removal of the primary LLC decreases the circulating angiogenesis inhibitor angiostatin, resulting in rapid growth of lung metastases (23). In mice treated with vehicle, there was marked growth of lung metastases (Figure (Figure7a).7a). The normal lung tissue was almost completely replaced by growing invasive metastases. The lung weights in these mice were 481 ± 85 mg (Figure (Figure7b).7b). In contrast, mice treated with rosiglitazone at 50 and 100 mg/kg/d showed no established invasive metastases (Figure (Figure7a),7a), with lung weights of 194 ± 22 and 165 ± 13 mg, respectively (Figure (Figure7b),7b), versus normal lung weights of 161 ± 8 mg (Figure (Figure77b).

Figure 7
Systemic therapy with PPARγ ligands prevents metastatic invasion after removal of primary LLC. (a) Visual comparison of mouse lungs on treatment day 17 with vehicle (Ctr) or rosiglitazone (R50, 50 mg/kg/d; R100, 100 mg/kg/d). Scale bar, 1 cm. ...

Individual LLC tumor cells in the rosiglitazone-treated mice were found inside the blood vessels, as demonstrated by hematoxylin-and-eosin staining (Figure (Figure7c).7c). To confirm that these cells were tumor cells, we performed immunofluorescence staining for pericentrin, a centrosomal protein used to detect neoplastic cells (34). LLC tumor cells in control lungs with invasive metastasis show a high level of centrosome abnormalities (>50%), as demonstrated by immunofluorescence staining for pericentrin (Figure (Figure7,7, d and e, insets). In rosiglitazone-treated mice, tumor cells with centrosome abnormalities were only located inside PECAM-stained lung blood vessels (Figure (Figure7,7, d and e). No LLC tumor cells were detected outside the vessels. These results suggest that rosiglitazone inhibits metastasis by preventing invasion of tumor cells through the endothelium.

It is widely appreciated that matrix metalloproteinases (MMPs) can promote tumor cell invasion while TIMPs decrease invasion. In order to determine whether rosiglitazone had an effect on tumor-associated MMP activity, we tested the conditioned media of endothelial cells that were treated with rosiglitazone via gelatin zymography. The predominant gelatinase detected was MMP-2 (gelatinase A), the activity of which appeared to be unaffected by rosiglitazone treatment (Figure (Figure7f).7f). Given that the net proteolytic activity is a function of the balance between MMPs and their endogenous inhibitors, the TIMPs, we next assayed these same samples in a radiometric enzyme assay for MMP inhibitory activity (25, 26). We found that rosiglitazone treatment resulted in an increase in MMP inhibitory bioactivity against the backdrop of approximately the same gelatinase activity (Figure (Figure7g).7g). Interestingly, this inhibitory profile exhibited the same biphasic response noted for the inhibition of endothelial cell proliferation and corneal neovascularization.


The role of PPARγ in tumors has been widely studied. PPARγ ligands have been reported to have direct effects on tumor cells. We show that, by inhibiting angiogenesis, PPARγ ligands may have clinical application in treating not only primary tumor growth but metastatic growth as well, independent of tumor cell PPARγ expression or direct TZD-induced inhibition of tumor cell proliferation.

Our proliferation studies show that endothelial and tumor cells display markedly different sensitivities to low doses of TZDs in vitro. The antiproliferative endothelial cell effects after 72 hours of treatment with 1–10 μM rosiglitazone are similar to those reported in HUVECs and choroidal endothelial cells (15, 18). Furthermore, at lower concentrations (0.01–0.1 μM) of rosiglitazone that correspond to the range of its affinity for binding PPARγ (30), we observed similar endothelial cell inhibition after 7 days. These concentrations also activate PPARγ in fibroblasts and adipocytes (27). Most PPARγ activation markers have been identified in adipocytes, such as adipocyte fatty acid–binding protein (aP2) (35); to date, none have been described for the endothelial cell system. Consequently, we used ligand-induced PPARγ degradation as a surrogate marker of activation. These results indicate that PPARγ is activated by its ligands in endothelial cells and suggest that the inhibition of proliferation of endothelial cells by TZDs may be a direct result of this activation. Importantly, the levels of rosiglitazone that inhibit endothelial proliferation are readily achieved in patients undergoing standard antidiabetic rosiglitazone treatment (36).

TZDs have been shown to inhibit tumor cell proliferation in a PPARγ-independent manner. In PPARγ-deficient embryonic stem cells, TZDs (25 μM) inhibit translation initiation by phosphorylation of eIF-2α (12). Rosiglitazone concentrations of 5 μM and higher led to phosphorylation of eIF-2α in HUVECs, suggesting that inhibition of proliferation of endothelial cells was mediated by a PPARγ-independent pathway. However, we observed that 0.01-1 μM of rosiglitazone, the concentration range at which PPARγ was activated, had the strongest antiproliferative effect on endothelial cells in vitro. Therefore, the inhibitory activity of rosiglitazone on endothelial cells is most likely mediated through PPARγ, whereas PPARγ-independent effects on translation may become important when higher concentrations of rosiglitazone are used.

In addition to direct action on endothelium, tumor angiogenesis can also be affected by indirect mechanisms. Our results showed that TZDs decreased VEGF production by tumor cells. Antiangiogenesis can result from a decrease of stimulators (e.g., VEGF and bFGF) and/or an increase of inhibitors (e.g., thrombospondin) in the tissue. It has been shown that PPARγ activation downregulates leptin and TNF-α, both of which are angiogenic factors (30, 37). Other reports show that PPARγ activation upregulates the expression of the angiogenesis inhibitor maspin and CD36, the receptor for antiangiogenic thrombospondin (5, 38, 39).

Antiangiogenic activity can also be mediated indirectly by pericytes and macrophages, which both express PPARγ. Pericytes (also known as mural cells) have recently been shown to be present in significant numbers in tumor blood vessels (40). Therefore, PPARγ ligands, which inhibit vascular smooth muscle cell proliferation and migration (30), may indirectly affect endothelial cell survival. Our CAM assay results suggest that PPARγ ligands have macrophage-independent effects in vivo. However, PPARγ ligands have been shown to inhibit macrophage activation and invasion, which are important modulators of tumor angiogenesis (30, 4143). Thus, PPARγ ligands may inhibit tumor angiogenesis by indirect as well as by direct mechanisms.

Surprisingly, higher doses of rosiglitazone (e.g., 400 mg/kg/d) were less antiangiogenic than lower doses (e.g., 50 mg/kg/d). Such a biphasic effect is not unprecedented, because other angiogenesis inhibitors, such as IFN-α, have less antiangiogenic activity at higher doses (20). This biphasic response is indicative of a negative feedback loop that operates at higher doses. One possibility is the drug-induced degradation of PPARγ, which at high dose might lead to complete depletion, and thus unresponsiveness. Alternatively, higher doses of rosiglitazone might induce enzymatic drug metabolism pathways. The results from twice-daily administration suggest that the doses of TZDs may be lowered further to achieve efficacy similar to that achieved with daily administration. Such a result is consistent with reports that frequent low doses of chemotherapy have increased antiangiogenic efficacy and that continuous administration of angiostatin increases tumor suppression at significantly reduced doses (29, 44, 45). This is presumably because endothelial inhibition is more related to duration of drug exposure than to peak levels achieved.

Several cancer cell lines, including bladder, breast, and thyroid carcinoma, require higher doses (50–100 μM) for inhibition of proliferation or are relatively resistant to antiproliferative effects of TZDs in vitro (5, 8, 10, 11, 46). Our tumor lines were minimally inhibited by rosiglitazone in vitro but were dramatically suppressed in vivo, in agreement with reports that TZDs have antitumor effects in PPARγ-negative tumors (12). Our antitumor effect resulted from a reduction in tumor microvessel density and a decrease in endothelial cell proliferation. Importantly, no signs of tumor cell differentiation or reduction in tumor cell proliferation were observed in treated tumors. This, together with the direct effects on the endothelium, suggests that the observed antitumor activity of TZDs is not solely mediated by a cell-autonomous response of the tumor cells.

In our studies, systemic PPARγ ligand therapy prevented metastatic invasion of LLC, consistent with the report that TZD administration inhibited the metastatic spread of thyroid tumors to the liver (11). Vascular invasion involves ECM proteolysis. Moreover, endothelial and tumor cells secrete proteinase inhibitors, such as TIMPs or plasminogen activator inhibitors (PAIs), which suppress tumor invasion and angiogenesis (26, 47). Our studies demonstrate that rosiglitazone increases the inhibition of MMP activity in HUVECs, and others have shown that PPARγ ligands can increase PAI-1 expression in human endothelial cells (14, 15). The mechanism by which PPARγ ligands such as rosiglitazone may prevent the establishment and progression of metastatic disease includes the previously described antiangiogenic effects such as inhibition of endothelial proliferation and decrease in VEGF secretion, in addition to the upregulation of negative regulators of metastatic invasion such as MMP inhibitors.

Our studies suggest that PPARγ ligands may be useful in treating angiogenic diseases such as cancer because of their effect on endothelium. Moreover, the endothelium has become an important target in the treatment of non-neoplastic diseases such as psoriasis, endometriosis, and arthritis. PPARγ ligands may represent a novel antiangiogenic therapy in rheumatoid arthritis (48). Furthermore, it is now becoming evident that multi-drug-resistant tumors can be effectively targeted by antiangiogenic chemotherapy (also called metronomic) chemotherapy (29, 45). As an orally administered FDA-approved drug used in over 2 million people with minimal side effects, rosiglitazone would be ideally suited for use in combination with other antiangiogenesis regimes and holds great promise to complement conventional modalities for cancer treatment.


We thank Carmen Barnes, Diane Bielenberg, Lynn Chang, Michael Fannon, Sui Huang, Mark Kieran, and Wei Wen for suggestions in preparing the manuscript. The excellent technical assistance of Geraldine Jackson, Andrea Laforme, Marty Olesiak, and Ricky Sanchez is acknowledged. We thank Kristin Gullage for photography. This study was supported by a sponsored research grant to Children’s Hospital from Entremed Inc. (Rockville, Maryland, USA). This work was supported by a European Molecular Biology Organization fellowship and by the Kopf Family Foundation (both to A. Kaipainen) and by NIH grant T32CA09535 (to D. Panigrahy).


Dipak Panigrahy and Samuel Singer contributed equally to this work.

Conflict of interest: No conflict of interest has been declared.

Nonstandard abbreviations used: thiazolidinedione (TZD); bovine capillary endothelial (BCE); human umbilical vein endothelial cell (HUVEC); Lewis lung carcinoma (LLC); green fluorescent protein (GFP); platelet/endothelial cell adhesion molecule (PECAM); prostatic-specific antigen (PSA); tissue inhibitor of metalloproteinase (TIMP); proliferating cell nuclear antigen (PCNA); chick chorioallantoic membrane (CAM); matrix metalloproteinase (MMP).


1. Rosen ED, Spiegelman BM. PPARγ: a nuclear regulator of metabolism, differentiation, and cell growth. J Biol Chem. 2001;276:37731–37734. [PubMed]
2. Barak Y, et al. PPAR-γ is required for placental, cardiac, and adipose tissue development. Mol Cell. 1999;4:585–595. [PubMed]
3. Tontonoz P, Hu E, Spiegelman BM. Stimulation of adipogenesis in fibroblasts by PPARγ 2, a lipid activated transcription factor. Cell. 1994;79:1147–1156. [PubMed]
4. Tontonoz P, Nagy L, Alvarez JG, Thomazy VA, Evans RM. PPARγ promotes monocyte/macrophage differentiation and uptake of oxidized LDL. Cell. 1998;93:241–252. [PubMed]
5. Mueller E, et al. Terminal differentiation of human breast cancer through PPARγ Mol Cell. 1998;1:465–470. [PubMed]
6. Sarraf P, et al. Differentiation and reversal of malignant changes in colon cancer through PPARγ Nat Med. 1998;4:1046–1052. [PubMed]
7. Tontonoz P, et al. Terminal differentiation of human liposarcoma cells induced by ligands for peroxisome proliferator-activated receptor γ and the retinoid X receptor. Proc Natl Acad Sci USA. 1991;94:237–241. [PubMed]
8. Elstner E, et al. Ligands for peroxisome proliferator-activated receptor γ and retinoic acid and receptor inhibit growth and induce apoptosis of human breast cancer cells in vitroand in BNX mice. Proc Natl Acad Sci USA. 1998;95:8806–8811. [PubMed]
9. Kubota T, et al. Ligand for peroxisome-activated receptor γ (Troglitazone) has potent antitumor effect against human prostate cancer both in vivo and in vitro. Cancer Res. 1998;58:3344–3352. [PubMed]
10. Nakashiro K, et al. Role of peroxisome proliferator-activated receptor γ and its ligands in non-neoplastic and neoplastic human urothelial cells. Am J Pathol. 2001;159:591–597. [PubMed]
11. Ohta K, Endo T, Haraguchi K, Hershman JM, Onaya T. Ligands for peroxisome proliferator-activated receptor γ inhibit growth and induce apoptosis of human papillary thyroid carcinoma cells. J Clin Endocrinol Metab. 2001;86:2170–2177. [PubMed]
12. Palakurthi SS, Aktas H, Grubissich LM, Mortensen RM, Halperin JA. Anticancer effects of thiazolidinediones are independent of peroxisome proliferator-activated receptor γ and mediated by inhibition of translation initiation. Cancer Res. 2001;61:6213–6218. [PubMed]
13. Folkman, J. 2000. Tumor angiogenesis. In Cancer medicine. 5th edition. J.F. Holland et al., editors. B.C. Decker Inc. Hamilton, Ontario, Canada. 132–152.
14. Marx N, Bourcier T, Sukhova GK, Libby P, Plutzky J. PPARγ activation in human endothelial cells increases plasminogen activator inhibitor type-1 expression: PPARγ as a potential mediator in vascular disease. Arterioscler Thromb Vasc Biol. 1999;19:546–551. [PubMed]
15. Xin X, Yang S, Kowalski J, Gerritsen ME. Peroxisome proliferator-activated receptor γ ligands are potent inhibitors of angiogenesis in vitro and in vivo. J Biol Chem. 1999;274:9116–9121. [PubMed]
16. Bishop-Bailey D, Hla T. Endothelial cell apoptosis induced by the peroxisome proliferator-activated receptor (PPAR) ligand 15-deoxy-prostaglandin J2. J Biol Chem. 1999;274:17042–17048. [PubMed]
17. Gralinski MR, Rowse PE, Breider MA. Effects of troglitazone and pioglitazone on cytokine-mediated endothelial cell proliferation in vitro. J Cardiovasc Pharmacol. 1998;31:909–913. [PubMed]
18. Murata T, et al. Peroxisome proliferator-activated receptor-γ ligands inhibit choroidal neovascularization. Invest Ophthalmol Vis Sci. 2000;41:2309–2317. [PubMed]
19. Inoue K, et al. Expression of peroxisome proliferator-activated receptor (PPAR)-gamma in human lung cancer. Anticancer Res. 2001;21:2471–2476. [PubMed]
20. Slaton JW, Perrotte P, Inoue K, Dinney C, Fidler IJ. Interferon-α-mediated down-regulation of angiogenesis-related genes and therapy of bladder cancer are dependent on optimization of biological dose and schedule. Clin Cancer Res. 1999;5:2726–2734. [PubMed]
21. D’Amato R, Loughnan MS, Flynn E, Folkman J. Thalidomide is an inhibitor of angiogenesis. Proc Natl Acad Sci USA. 1994;91:4082–4085. [PubMed]
22. Masferrer JL, et al. Antiangiogenic and antitumor activities of cyclooxgenase-2 inhibitors. Cancer Res. 2000;60:1306–1311. [PubMed]
23. O’Reilly MS, et al. Angiostatin: a novel angiogenesis inhibitor that mediates the suppression of metastases by a lewis lung carcinoma. Cell. 1994;79:315–328. [PubMed]
24. Stephenson RA, et al. Metastatic model for human prostate cancer using orthotopic implantation in nude mice. J Natl Cancer Inst. 1992;84:951–957. [PubMed]
25. Braunhut S, Moses M. Retinoids modulate endothelial cell production of matrix-degrading proteases and tissue inhibitors of metalloproteinases (TIMP) J Biol Chem. 1994;269:13472–13479. [PubMed]
26. Moses MA, Sudhalter J, Langer R. Identification of an inhibitor of neovascularization from cartilage. Science. 1990;248:1408–1410. [PubMed]
27. Hauser S, et al. Degradation of the peroxisome proliferator-activated receptor γ is linked to ligand dependent activation. J Biol Chem. 2000;275:18527–18533. [PubMed]
28. Moses MA, et al. Troponin I is present in human cartilage and inhibits angiogenesis. Proc Natl Acad Sci USA. 1999;96:2645–2650. [PubMed]
29. Browder T, et al. Antiangiogenic scheduling of chemotherapy improves efficacy against experimental drug-resistant cancer. Cancer Res. 2000;60:1878–1886. [PubMed]
30. Berger J, Moller DE. Mechanism of action of PPARs. Annu Rev Med. 2002;53:409–435. [PubMed]
31. Ribatti D, Vacca A, Roncali L, Dammacco F. The chick embryo chorioallantoic membrane as a model for in vivoresearch on antiangiogenesis. Curr Pharm Biotechnol. 2000;1:73–82. [PubMed]
32. Folkman J. Angiogenesis-dependent diseases. Semin Oncol. 2001;28:536–542. [PubMed]
33. Hlatky L, Hahnfeldt P, Folkman J. Clinical application of antiangiogenic therapy: microvessel density, what it does and does not tell us. J Natl Cancer Inst. 2002;94:883–893. [PubMed]
34. Pihan GA, et al. Centrosome defects and genetic instability in malignant tumors. Cancer Res. 1998;58:3974–3985. [PubMed]
35. Elbrecht A, et al. Molecular cloning, expression and characterization of human peroxisome proliferator activated receptors γ1 and γ2. Biochem Biophys Res Commun. 1996;224:431–437. [PubMed]
36. Freed MI, Allen A, Jorkasky DK, DiCicco RA. Systemic exposure to rosiglitazone is unaltered by food. Eur J Clin Pharmacol. 1999;55:53–56. [PubMed]
37. Sietta-Honigmann MR, et al. Biological action of leptin as an angiogenic factor. Science. 1998;281:1683–1686. [PubMed]
38. Zhang M, Volpert O, Shi YH, Bouck N. Maspin is an angiogenesis inhibitor. Nat Med. 2000;6:196–199. [PubMed]
39. Jimenez B, et al. Signals leading to apoptosis-dependent inhibition of neovascularization by thrombospondin-1. Nat Med. 2000;6:41–48. [PubMed]
40. Morikawa S, et al. Abnormalities in pericytes on blood vessels and endothelial sprouts in tumors. Am J Pathol. 2002;160:985–1000. [PubMed]
41. Sunderkotter C, Steinbrink K, Goebeler M, Bhardwaj R, Sorg C. Macrophages and angiogenesis. J Leukoc Biol. 1994;55:410–422. [PubMed]
42. Ricote M, Li AC, Willson TM, Kelly CJ, Glass CK. The peroxisome proliferator-activated receptor-γ is a negative regulator of macrophage activation. Nature. 1998;391:79–82. [PubMed]
43. Pasceri V, Wu HD, Willerson JT, Yeh ETH. Modulation of vascular inflammation in vitro and in vivo by peroxisome proliferator-activated receptor-γ activators. Circulation. 2000;101:235–238. [PubMed]
44. Drixler TA, et al. Continuous administration of angiostatin inhibits accelerated growth of colorectal liver metastases after partial hepatectomy. Cancer Res. 2000;60:1761–1765. [PubMed]
45. Klement G, et al. Continuous low-dose therapy with vinblastine and VEGF receptor–2 antibody induces sustained tumor regression without overt toxicity. J Clin Invest. 2000;105:15–24. [PMC free article] [PubMed]
46. Clay CE, et al. Magnitude of peroxisome proliferator-activated receptor-gamma activation is associated with important and seemingly opposite biological responses in breast cancer cells. J Investig Med. 2001;49:413–420. [PubMed]
47. Liotta LA, Steeg PS, Stetler-Stevenson WG. Cancer metastasis and angiogenesis: an imbalance of positive and negative regulation. Cell. 1991;64:327–336. [PubMed]
48. Fahmi H, Pelletier JP, Martel-Pelletier J. PPARγ ligands as modulators of inflammatory and catabolic responses in arthritis. An overview. J Rheumatol. 2002;29:3–14. [PubMed]

Articles from The Journal of Clinical Investigation are provided here courtesy of American Society for Clinical Investigation