Background
The Hedgehog family of genes encodes secreted signaling molecules that regulate cell proliferation and cell fate determination. In mammals, there are three such genes: Sonic hedgehog (
Shh), Indian hedgehog (
Ihh), and Desert hedgehog (
Dhh). All three Hedgehog (Hh) proteins function by binding to the transmembrane receptor, Patched-1 (Ptc-1), leading to the de-repression of the membrane-bound inhibitor, Smoothened [
1,
2]. This results in activation of the transcription factor Gli-1, which induces expression of target genes that include Ptc-1 and Gli-1 itself. The increase in expression of Ptc-1 may limit the range of action of Hh by sequestering it at the surface of Hh-responsive cells [
3].
Hedgehog-interacting protein (HIP) was discovered by screening a mouse cDNA expression library for proteins that bound to Shh [
4]. HIP binds all three Hh proteins with an affinity equal to that of Ptc-1, and in mouse embryos it is expressed in cells adjacent to those expressing Shh, positioning it appropriately for in vivo interactions. Ectopic expression of Shh leads to ectopic HIP expression, indicating that HIP is a transcriptional target of Hh signaling [
4]. Transgenic mice that overexpress HIP in the endochondral skeleton displayed a phenotype similar to that of Ihh knockout mice, consistent with an inhibitory role for HIP in Hh signaling [
4]. Although it has been shown that overexpression of HIP in cells making Shh reduced the amount of Shh secreted into the media [
5], no data has been published specifically demonstrating that expression of HIP in responding cells inhibits the activation of the Shh signaling pathway.
During gastrulation in the mouse, Ihh is secreted by the endoderm and is sufficient to activate hematopoiesis and vasculogenesis [
6]. In addition to its role in developmental processes, Shh was shown to induce angiogenesis in a murine corneal angiogenesis model, probably through the induction of the angiogenic factors VEGF, Ang-1, and Ang-2 [
7]. Moreover, inhibition of Shh in the ischemic hindlimb of mice through the use of a neutralizing antibody inhibits endogenous angiogenesis [
8]. Hh is also required for normal angiogenesis in the murine yolk sac, as Ihh
-/- mice can initiate vasculogenesis and hematopoiesis but are defective in vascular remodeling to form blood vessels [
9]. In the murine cornea, fibroblasts were identified as the Shh-responsive cells, while endothelial cells in the corneal neovessels, as well as human umbilical vein endothelial cells and microvascular endothelial cells cultured
in vitro, were unable to respond to Shh, even though they express the receptor Ptc-1 [
7].
Misregulation of the Hh signaling pathway has been implicated in several different types of cancer, including basal cell carcinomas (BCCs), medullablastomas, and gliomas (reviewed in [
10]. Mutations in Ptc-1, which lead to constitutive activation of the Hh pathway, are the underlying factor in basal cell nevus syndrome, a familial condition characterized by a predisposition to BCC development [
11]. In addition, Gli-1 was originally identified as a gene overexpressed in a human glioma line [
12]. Recently, it was reported that Hh pathway activity is upregulated in digestive tract, pancreatic, and small-cell lung tumors and is required for the growth of these tumors [
13‐
15].
Here we show that overexpression of HIP in cultured mouse Leydig cells inhibits the ability of these cells to respond to exogenous Shh, confirming that HIP can block Hh signaling when expressed in the same cells as the receptor Ptc-1. We have also shown that HIP is expressed predominantly in vascular endothelial cells and is downregulated in HUVEC during in vitro angiogenesis. Strikingly, HIP mRNA levels were decreased or even absent in several types of human tumors, as well as in highly vascularized human tumors grown in nude mice. Taken together, these results indicate a correlation between angiogenesis and decreased expression of HIP, lending support to the role of HIP as a naturally occurring regulator of Hh signaling and neovessel formation in the adult organism.
Methods
Adherent cultures of 293-EBNA cells were transfected with a Shh-pCDNA3 expression plasmid kindly provided by Dr. Pao-Tien Chuang (UCSF) using LipofectAMINE 2000 and OptiMem reduced-serum medium (Invitrogen). Three to five hours after transfection, cells were re-fed with serum-containing growth medium, and three or four days later conditioned medium was collected and filtered through 0.2-μm cellulose acetate filters.
For RNA isolation, human aortic endothelial cells (HAEC) were cultured in 12-well plates with or without Matrigel (BD Biosciences) for 16 hours, then cells were lysed, digested with proteinase K, and total RNA was extracted using the RNeasy Mini Kit (Qiagen). HIP expression was assayed by real-time quantitative reverse transcriptase PCR (Q-RT-PCR) and normalized to 18s rRNA (see below).
Transfection and conditioned medium assays
The mouse testicular epithelial cell line, TM3, was grown in complete medium (DMEM/F12 with 2.5% FBS, 5% horse serum, 15 mM Hepes, and 4 mM glutamine) at 37°C and 5% CO2. Cells were transfected in 12-well or 24-well plates at 80–90% confluence using LipofectAMINE 2000 transfection reagent and OptiMem reduced-serum medium (Invitrogen). For conditioned medium (CM) assays, cells were transfected with the plasmid MycHIP-pCDNA3 (gift of Dr. Pao-Tien Chuang, UCSF), which encodes full-length mouse HIP, or empty vector (mock). Mock or Shh CM was added to cells 36 hours after transfection, then RNA was harvested 36–48 hours later.
Collection of mouse tissues
PC3 human prostate cancer cells were implanted subcutaneously into male nude mice (strain nu/nu), and on day 39 the resulting tumors were excised, weighed, placed on dry ice, then stored at -80°C prior to RNA isolation. A549 lung cancer cells were implanted subcutaneously into female nude mice and harvested as described above on day 9. Normal livers or skin from 5- to 6-week-old male or 4- to 5-week-old female nude mice were excised immediately following cervical dislocation and frozen in liquid nitrogen, then stored at -80°C.
RNA isolation
RNA was extracted from cultured cells using the RNeasy kit (Qiagen), including on-column DNase I digestion, according to the manufacturer's instructions. To extract RNA from frozen normal mouse tissues and tumors, hard-frozen tissue samples of 100–300 μg were pulverized over dry ice, placed in denaturing buffer, and disrupted using a Mixer Mill (Retsch) or rotor-stator homogenizer (Omni International). RNA was isolated from the homogenate either by phenol-chloroform extraction followed by precipitation with isopropanol and washing with 70% ethanol (ToTALLY RNA kit, Ambion) or by using the RNeasy kit (Qiagen). All RNA samples were treated with DNase I (Qiagen) prior to quantitative RT-PCR. Concentrations of RNAs were determined by reading the absorbance at 260 nm.
Quantitative RT-PCR
Quantitative RT-PCR was performed using the ABI PRISM™ 7700 Sequence Detection System and TaqMan™ chemistry. Reactions contained 0.3 μM of each primer, 0.1 μM probe, 0.25 U/ml MultiScribe reverse transcriptase, 0.4 U/ml RNase inhibitor, and 1x PCR master mix (Applied Biosystems). Primers and probes used to quantitate the mRNA level of various genes were as follows: mouse Ptc-1 (forward primer 5'GCCAATGGCCTAAACCGACT, reverse primer 5'AAACCGGACGACACTTGGAG, probe 5'6FAM-CCCACTCCTTCGCCTGAGCCG-TAMRA), mouse HIP (forward primer 5'CCACTGACCTCCGATTGCTC, reverse primer 5'TGCAGCAGCACTTGCCAG, probe 5'6FAM-CGGCTCTGTCGAAACGGCTACTACACC-TAMRA), mouse vWF (forward primer 5'CCGGAAGCGACCCTCAGA, reverse primer 5'CGGTCAATTTTGCCAAAGATCT, probe 5'6FAM-TGGCCTCTACCAGTGAGGTTTTGAAGTACACAC-TAMRA), mouse CD146 (forward primer 5'GGGCCTCAGGCAACTTCA, reverse primer 5'TTGGTGCACACGGAAAATCA, probe 5'6FAM-CTCCTTGTGAATCAAAAACCAGTCCACTTGG-TAMRA), human HIP (forward primer 5'CCCACACTTCAACAGCACCA, reverse primer 5'GCACATCTGCCTGGATCGT, probe 5'6FAM-CCCCGAAGTGTTTGCTCATGGGCT-TAMRA), human vWF (forward primer 5'TGAAGTATGCGGGCAGCC, reverse primer 5'GCGGTCGATCTTGCTGAAG, probe 5'6FAM-CCTCCACCAGCGAGGTCTTGAAATACAC-TAMRA). Mouse and human GAPDH and ribosomal RNA probe and primer sets were purchased from Applied Biosystems. RNA quantities were determined from a standard curve of serially diluted total cellular or tissue RNA run in parallel with each set of reactions. Standard curves had a slope between -3.1 and -3.3 and correlation coefficients of 0.98 or greater.
Western blot
Total cell lysates were made by lysing cells in 2% SDS, 10% glycerol, and 0.063 M Tris-HCl (pH 6.8) containing a cocktail of protease inhibitors (Pierce). Lysates were heat denatured at 95°C for 10 minutes, passed through a 26G needle to shear DNA, and centrifuged at 10,000 g for 30 minutes to remove insoluble material. Protein concentrations were determined using the BCA assay (Pierce). Conditioned medium samples were diluted 1:1 in Laemmli sample buffer (Sigma). 50 μg of cell lysate or 20 μl of conditioned medium/sample buffer was resolved on 4–15% polyacrylamide gels (BMA) and transferred to nitrocellulose (Invitrogen). Even loading of protein samples was verified by staining with Ponceau S. After overnight blocking with 5% nonfat dry milk, 0.05% Tween-20 in phosphate-buffered saline, blots were incubated with antibodies against Shh (sc-1194, Santa Cruz), Myc tag (Invitrogen), or HIP (provided by Dr. Pao-Tien Chuang, UCSF). Antibody-antigen complexes were visualized using horseradish peroxidase-conjugated secondary antibodies (Jackson ImmunoLabs, Santa Cruz) and SuperSignal West Pico chemiluminescent substrate (Pierce).
Hybridization of RNA probes to cancer array
Linearized templates containing a 716-bp fragment of human HIP cDNA (bases 521–1236 of human HIP coding sequence) or a 777-bp fragment of human vWF cDNA (bases 7301–8077 of human vWF coding sequence) were radiolabelled with 32P-dUTP by in vitro transcription using the MAXIscript kit (Ambion). The array was pre-hybridized in Clontech ExpressHyb solution with 100 μg/ml boiled, sheared salmon testis DNA (SS-DNA) for 2–12 hours at 68°C with rotation. Pre-hybridization solution was replaced with fresh hybridization solution with SS-DNA, plus a total of 1.5–1.7 × 107 cpm of 32P-labelled HIP or vWF probe. Hybridization of the probe proceeded for 16–18 hours at 68°C, followed by four washes in 2X SSC/0.5% SDS at 68°C, one wash in 0.2X SSC/0.5% SDS at 68°C, and one wash in 2X SSC at room temperature. The array was exposed to a phosphor-screen for 24–72 hours and scanned in a Storm phosphor-imager at a resolution of 50 μm. After hybridization to the HIP probe, the same array was stripped by boiling in 0.5% SDS and re-scanned to verify the absence of residual probe before hybridization to the vWF probe. Relative levels of HIP and vWF expression were determined using ImageQuant software (Molecular Dynamics).
Statistical analysis
All results are expressed as mean ± standard deviation unless otherwise noted. Statistical significance of differences was determined using a two-tailed Student's t-test.
Discussion
Our demonstration that HIP functions to inhibit Ptc-1 upregulation in mouse testicular epithelial cells (TM3) exposed to Shh-containing conditioned media is the first direct evidence to date that Shh signaling is attenuated in cells that express full-length, membrane-bound HIP. The decrease in Ptc-1 induction caused by transfection with HIP is consistent with previous reports indicating that HIP can bind and reduce the availability of Shh and presumably prevent it from signaling through Ptc-1 [
4,
5]. In human aortic endothelial cells (HAEC), which express high levels of HIP, the addition of Shh-containing conditioned medium did not cause induction of Ptc-1, even though these cells express the receptor components Ptc-1 and Smo. In addition, others have shown that although Shh induces angiogenesis in a mouse model of hindlimb ischemia, it has no effect on endothelial cell proliferation or migration in cell culture [
7]. Our finding that vascular EC express abundant amounts of HIP mRNA may explain the inability of these cells to respond to Shh. An analysis of various human cell lines and primary cells indicated that HIP is absent or expressed at low levels in other cell types, suggesting that in adults HIP is expressed primarily in EC. These results are supported by gene chip data analysis of more than 30 normal human tissues showing that HIP is most highly expressed in blood vessels or in vascular-rich tissues such as liver, lung, brain, and pancreas (data not shown). These results suggest a role for HIP in the normal function of blood vessels.
Several lines of evidence support the hypothesis that HIP expression is decreased in EC participating in angiogenesis. Firstly, we describe that HIP is downregulated in HAEC forming tubes on Matrigel. In contrast, Ptc-1 mRNA levels were increased in EC forming tubes on Matrigel, suggesting that the decrease in HIP mRNA under these conditions does not reflect a general downregulation of Hh-responsive genes. Given that transcription of HIP and Ptc-1 are both activated by Hh signaling, it is likely that the decrease in HIP expression in EC on Matrigel is mediated by a pathway independent of Hh signaling. Secondly, we have observed that HIP mRNA levels are decreased in human tumors and xenograft human tumors grown in mice, situations in which angiogenesis occurs. Previous studies have demonstrated a requirement for Shh in angiogenesis in the ischemic mouse limb and embryonic yolk sac [
8,
9]. The pro-angiogenic activity of exogenously supplied Shh protein has been attributed to the induction of factors such as VEGF and angiopoietin in fibroblasts [
7]. Our data suggest the possibility that in situations where HIP expression is downregulated, Hh may also act directly on endothelial cells.
The Shh pathway has been implicated in several different types of cancer, where upregulation of signaling, associated with mutations in Patched or amplification of Gli, is often the suspected cause of malignancy [
11,
12,
24‐
26]. In at least one type of human cancer, basal cell carcinoma (BCC), HIP upregulation has been demonstrated [
27,
28], probably as a result of dysregulation of the Shh signaling pathway. More recently it has been reported that Hh pathway activity is activated in a wide variety of digestive tract tumors by overexpression of the Hh ligand, and is essential for tumor growth [
13]. Aberrant expression of Shh and activation of Hh signaling was also demonstrated to occur in pancreatic cancer [
14] and small cell lung cancer [
15]. Hh ligands secreted by tumor cells have the potential to induce Hh pathway activation in nearby non-tumor cells, including fibroblasts and endothelial cells. Our observation that HIP mRNA expression decreases in several human tumor types relative to normal tissues suggests that modulation of HIP expression may also promote increased Hh signaling in certain tumors and contribute to cancer progression. However, since expression of HIP is known to be induced by activation of the Hh pathway, an alternative interpretation is that a reduced level of HIP mRNA in tumors is indicative of reduced Hh signaling, as suggested by Hu et al. [
29]. Our finding that, in endothelial cells in Matrigel, HIP mRNA levels decrease while Ptc-1 levels increase demonstrates that a mechanism other than Hh signaling can modulate the expression of these Hh target genes. Thus, the down-regulation of HIP in tumors may be unrelated to Hh pathway activity. The precise mechanism of HIP regulation by the Hh pathway in the context of tumors remains to be elucidated by future studies. Among the tumor types represented on the Clontech Cancer Profiling Array, liver and several areas of the digestive tract (stomach, colon, rectum) exhibited consistent downregulation of HIP in the tumor relative to normal tissue. Tumors from other tissues, including breast, testis, and kidney, did not show a significant change in HIP expression from the normal tissue, suggesting that this phenomenon may be restricted to certain tumor types. Differences in the degree of vascularization of the various tumors may also explain why a decrease in HIP was not seen in all tumor types.
Xenotransplantation of PC3 or A549 cells into immunocompromised mice is a commonly used animal model for prostate or lung cancer, respectively. Extensive neovascularization occurs in the resulting tumors, and it has been demonstrated that angiogenesis inhibitors slow their growth [
30,
31]. The discovery that vWF-normalized mouse HIP mRNA levels were markedly decreased in A549 tumors and undetectable in all of the PC3 tumors we examined gives further weight to the hypothesis that decreased HIP expression is associated with tumor angiogenesis.
Angiogenesis has been well-characterized as a prerequisite to continued tumor growth and metastasis [
16,
17,
32], and many approaches have been developed to attempt to control the progression of cancer by inhibiting angiogenesis [
32,
33]. A more complete analysis of the gene expression changes in endothelial cells during developmental and pathological processes should help to identify additional signaling pathways that are altered and that could be manipulated to control angiogenesis and disease progression. The identification of Shh as an angiogenic signaling molecule [
7], along with the characterization of HIP as an inhibitor of Shh that is downregulated in certain tumors, strongly suggests that inhibition of the Shh pathway may be of therapeutic use in various cancers that rely on angiogenesis for their continued growth.
Conclusions
We have shown that HIP is expressed predominantly in EC but at low or undetectable levels in other cell types, and that the high expression of HIP in EC may be responsible for their inability to respond to Shh. Expression of HIP in TM3 cells attenuated their response to Shh, demonstrating that HIP antagonizes Hh signaling when expressed in the responding cell. The reduction of HIP in a variety of human tumor samples as well as PC3 and A549 xenograft tumors, and in EC undergoing tube formation on Matrigel, suggests that modulation of HIP may play a role in tumor angiogenesis.
Acknowledgements
We are grateful to Dr. Pao-Tien Chuang for providing HIP expression vectors and helpful advice. We thank Ying Zhu and Wei Xia for help with protein expression, Bruno Alicke for providing mouse tissues, and Rhonda Humm, Eileen Paolo-Chrisco, and Jean MacRobbie for cell culture assistance. We also thank Rick Harkins for helpful discussions on the research and the manuscript.
Authors' contributions
CLO participated in experimental design and carried out CM production and assays, tissue and RNA processing, Q-RT-PCR, Western blot, and cancer array hybridization. PPH participated in the design of the study and performed tube formation assays, tissue and RNA processing, Q-RT-PCR, and Western blot. JG participated in initial characterization of HIP and provided supporting data. GMR was involved in the planning and organization of the study and reviewed the manuscript. ARB initiated, planned, and supervised the entire study.