Introduction
Angiogenesis is a key requirement for tumour growth (
Folkman, 1995;
Chung et al, 2010). Much evidence indicates that VEGF is a major regulator of angiogenesis (
Chung and Ferrara, 2011). Various inhibitors of the VEGF signalling pathway have been developed and approved for treatment of cancer or intraocular neovascular disorders (
Ferrara et al, 2007;
Ebos and Kerbel, 2011). Recently, microRNAs (miRNAs) have been shown to provide a new layer of regulation of gene expression in many physiological and pathological processes, including angiogenesis (
Wang and Olson, 2009;
Anand and Cheresh, 2011;
Small and Olson, 2011;
Weis and Cheresh, 2011).
miRNAs are a family of noncoding RNAs ∼22 nt in length, which can suppress gene expression by pairing to the 3′ untranslated regions (UTRs) of target mRNAs (
Bartel, 2004,
2009). Accumulating evidence indicates that endothelial miRNAs are involved in developmental and tumour angiogenesis, thus providing opportunities for further control of the tumour vasculature. Ablation of the miRNA precursor‐processing enzyme Dicer in endothelium reduces tumour angiogenesis and progression (
Suarez et al, 2008), suggesting that specific miRNAs in endothelial cells regulate angiogenic processes. In this regard, miR‐296 and miR‐132, both induced by VEGF, have been proposed to facilitate angiogenic switching (
Wurdinger et al, 2008;
Anand et al, 2010). It would be of considerable interest to identify VEGF‐independent angiomirs, which might serve as anti‐angiogenic targets in combination with current anti‐VEGF therapies.
We performed a quantitative PCR‐based miRNA screen and identified a set of differentially expressed miRNAs in microvascular endothelial cells co‐cultured with tumour cells. Unexpectedly, most miRNAs were derived from tumour cells, packaged into microvesicles (MVs), and then directly delivered to endothelial cells. Tumour secreted miRNAs were functional in recipient endothelial cells as assessed by the ability to promote migration and neovascularization. Thus, our data support a novel cellular communication involving directional transfer of miRNAs during tumour angiogenesis.
Discussion
We systematically profiled endothelial miRNAs significantly changed by tumour cells in our co‐culture system and discovered a subset of miRNAs directly transferred from tumour to endothelial cells. Furthermore, we describe a novel role of miR‐9 in regulating tumour angiogenesis by modulating the JAK‐STAT pathway in endothelial cells. These findings support the hypothesis that tumour‐secreted miRNAs constitute a molecular mechanism implicated in the regulation of tumour neovascularization.
Previous studies have shown that miRNAs are stably detectable in human bloodstream and that alterations in circulating miRNAs are associated with certain cancers (
Mitchell et al, 2008;
Zhu et al, 2009;
Komatsu et al, 2011;
Mostert et al, 2011). Therefore, miRNAs may represent novel non‐invasive biomarkers for cancer diagnosis (
Mitchell et al, 2008;
Hu et al, 2010;
Boeri et al, 2011;
Liu et al, 2011). Several investigations suggest that tumour‐derived miRNAs enter the circulation predominantly through tumour‐released MVs/exosomes (
Kosaka et al, 2010;
Muralidharan‐Chari et al, 2010;
Grange et al, 2011). Our data further indicate that tumour‐derived miRNAs may be packaged into specific populations of MVs and function as important mediators of tumour‐stroma communication.
The finding that endothelial‐targeting miRNAs are within a heparin‐binding complex is particularly intriguing. It is well established that heparan sulphate proteoglycans are widely distributed in the extracellular matrix (ECM) and that interactions with such moieties are of fundamental importance for a variety of processes, including angiogenesis (
Munoz and Linhardt, 2004). Heparin binding is known to facilitate targeting of angiogenic molecules to the ECM and cell surface of endothelial cells (
Munoz and Linhardt, 2004). Also, other studies have shown that, once bound to heparin, growth factors may become much more stable and resistant to degradation induced by various agents (
Gospodarowicz and Cheng, 1986). All of these properties might be crucially important for MV stability and miRNA functions described in our study. Further biochemical characterization of this complex is necessary to elucidate the biological significance of our observation.
It is noteworthy that MV‐mediated delivery, as observed for miR‐9, is unlike the mechanism of endothelial up‐regulation of miR‐296 and miR‐132, which have been characterized as positive regulators of angiogenesis. Both miRNAs have been reported to be upregulated by VEGF in endothelial cells (
Wurdinger et al, 2008;
Anand et al, 2010). In our co‐culture screens, miR‐296 and miR‐132 were induced by some but not all tumour cell lines, with much lower fold changes compared to miR‐9. Furthermore, other miRNAs have been shown to regulate endothelial cell recruitment indirectly, through modulation of expression of angiogenic factors within tumour cells (
Dews et al, 2006;
Png et al, 2012). Therefore, during angiogenesis delivery of genetic information mediated by miRNAs may occur through multiple mechanisms. It remains to be determined whether different tumours preferentially choose one or other mechanism and how these miRNAs are coordinated in regulating angiogenesis.
Our data implicate miR‐9 in endothelial biology and tumour angiogenesis. miR‐9 is increased in breast cancer and many other tumour types (
Ma et al, 2010;
Shigehara et al, 2011). It has been reported that miR‐9 promotes tumour cell motility and metastasis by repressing E‐cadherin expression. In the present study, we found that miR‐9 also enhances endothelial cell migration and angiogenesis. Although miR‐9 was proposed to increase
vegf transcription in tumour cells (
Ma et al, 2010), our results suggested that this is not a universal mechanism since miR‐9 knockdown did not induce
vegf mRNA changes in any of the tumour cell lines we tested. On the other hand, miR‐9 was consistently upregulated in tumour‐associated endothelial cells, which resulted in reduced SOCS5, a predicted target of miR‐9. Consequently, the JAK‐STAT signalling cascade was aberrantly activated. Therefore, it is tempting to speculate that miR‐9, similar to miR‐17‐92 cluster (
Olive et al, 2010), acts as a potent oncomir by simultaneously activating multiple tumorigenic pathways.
The JAK‐STAT pathway is recognized as one of the major oncogenic signalling pathways activated in a variety of human malignancies (
Yu and Jove, 2004). STAT proteins not only play a crucial role in tumour cell proliferation, survival and invasion, but also significantly contribute to the formation of a unique tumour microenvironment (
Lee et al, 2009;
Yu et al, 2009). A link between STATs activation in endothelial cells and tumour angiogenesis has been described in several studies (
Bartoli et al, 2003;
Leong et al, 2009;
Dong et al, 2010). In addition, JAK1 was identified as an endothelial miR‐17‐92 target and was functionally validated as a proangiogenic molecule (
Doebele et al, 2010), providing a rationale for targeting this pathway. Intriguingly, our data indicate that miR‐9 prominently triggers JAK‐STAT activities, and that inhibition of both JAK1 and JAK2 is sufficient to abrogate the effects. These findings highlight the importance of understanding the major target of miRNAs and suggest that, although it is challenging to therapeutically inhibit miR‐9 in patients, JAK inhibitors might be an alternative approach. Indeed, we show that a JAK2 inhibitor efficiently blocked miR‐9‐induced pSTAT1 and pSTAT3. As a result, endothelial cell migration and tumour burden in mice were significantly reduced. In agreement with our findings, a recent study demonstrated that another JAK2 inhibitor also reduced tumour growth, as least in part through inhibition of angiogenesis (
Xin et al, 2011). Of note, several JAK inhibitors are currently in late‐stage trials for treating different diseases and generally have shown acceptable toxicological profiles (
Garber, 2011).
Tumour angiogenesis is a complex process, requiring the involvement of multiple mediators. The present study extends our understanding of how this process is regulated by tumour‐secreted miRNAs, which represent a new class of modulators in recipient endothelial cells. Further characterization of intercellular miRNA communication and downstream signalling events would help us identify novel mechanisms of angiogenesis and develop new therapeutic strategies.
Materials and methods
Cell culture
Primary microvascular endothelial cells from human brain, colon, and pancreas and HUVECs were purchased from Lonza (Walkersville, MD). Human dermal and lung microvascular endothelial cells were from Cell Systems (Kirkland, WA). Endothelial cells were cultured in EGM‐2 or EGM‐2MV medium (Lonza). Tumour cell lines were obtained from the Genentech cell line repository (gCell) and were cultured in DMEM (high glucose) supplemented with 10% fetal bovine serum (Invitrogen). The HM7 cell line is a variant of LS 174T human colorectal carcinoma cell line, as previously described (
Bresalier et al, 1991;
Warren et al, 1995). Tumour‐endothelial co‐culture experiments were performed in six‐well plates with 8‐micron inserts (BD Biosciences). miRNA mimics (Applied Biosystems) and siRNA sequences (Dharmacon) were transfected with Lipofectamine RNAiMAX reagent (Invitrogen).
miRNA profiling and quantitative PCR
Total RNA was prepared with mirVana miRNA isolation kit (Ambion) according to manufacturer's protocol. miRNA in 500 ng total RNA was subjected to reverse transcription using the Megaplex RT primer pools and the Taqman microRNA reverse transcription kit (Applied Biosystems). The resultant cDNA was pre‐amplified using Megaplex PreAmp primers and TaqMan PreAmp master mix (Applied Biosystems), and then loaded into the Taqman array microRNA cards. The real‐time PCR was run on the Applied Biosystems 7900HT machine. Relative expression levels of each miRNA were normalized to U6 snRNA. Expression of individual miRNAs was quantified by TaqMan miRNA assays (Applied Biosystems) following manufacturer's instructions. U6 snRNA was used as the endogenous control for all experiments. At least three biological replicates were included for each condition.
Cell migration assay
Real‐time monitoring of endothelial cell migration was performed using the xCELLigence system with the CIM‐Plate 16 (Roche). The upper chamber was coated with 20 μg/ml Fibronectin (BD Biosciences) and seeded with 50 000 HUVECs. When cells migrated through the membrane into the bottom chamber in response to attractants, they contacted and adhered to the electronic sensors, resulting in an increase in impedance. The cell‐index values reflecting impedance changes were automatically and continuously recorded every 15 min.
HUVEC sprouting assay
Twenty hours after transfection, HUVECs were mixed with Cytodex microcarrier beads (Sigma‐Aldrich) in a ratio of 106 cells per 2500 beads and incubated for 4 h at 37°C. Coated beads were then cultured in a six‐well dish overnight. The following day, ∼200 coated beads were dissolved in a solution of 2 mg/ml fibrinogen (Sigma‐Aldrich) in EGM‐2, and added to 0.625 U/ml of thrombin (Sigma‐Aldrich) in one well of a 24‐well plate. Skin fibroblasts (D551) were then plated on top of the clot and incubated with D551 conditioned medium and EGM‐2 (3:1). HUVEC sprouts were visualized by immunostaining with Alexa Fluor 488 phalloidin (1:100) and Hoecsht 33258 (1:1000) (Invitrogen) overnight at 4°C. Image Xpress Micro was used for capturing images and HUVEC sprouting was analysed in MetaXpress software.
MV isolation
Tumour cells were cultured in serum‐free DMEM. Conditioned medium was collected after 48 h and concentrated 10‐fold. MVs were isolated using two independent methods. For differential centrifugation, conditioned medium was filtered through a 0.22‐μm membrane and centrifuged for 30 min at 16 500 g. Supernatants were filtered again and MVs were pelleted by ultracentrifugation for 2 h at 110 000 g. In the other approach, ExoQuick precipitation reagent (System Biosciences) was mixed with concentrated conditioned medium and MVs were precipitated by centrifugation.
Chromatography
Approximately 80% confluent SK23 cells were incubated in serum‐free medium for 3 days. Conditioned media were collected and concentrated 10‐fold as starting material for chromatography. The heparin‐sepharose column (Hi‐Trap, HS, 5 ml) was pre‐equilibrated with 20 mM Tris, pH 7.4. The Hi‐Trap Q sepharose column, 1 ml (GE Healthcare) was pre‐equilibrated with 20 mM Tris, pH 8.0. Samples were injected into the column and bound material was eluted with a linear gradient of NaCl. Aliquots of fractions were tested on HUVECs for miR‐9 expression.
Western blot
Cells were lysed in RIPA buffer (Tris pH 7.4 50 mM, NaCl 150 mM, NP‐40 1%, SDS 0.1%, EDTA 2 μM) containing proteinase inhibitors (Roche) and phosphatase inhibitors (Sigma). The cell lysates (20 ug protein) were subjected to SDS–PAGE and western blot. Antibodies against the following proteins were used: pTyr‐701 STAT1, STAT1, pTyr‐705 STAT3, STAT3, pTyr‐1022/1023 JAK1, JAK1, pTyr‐1007/1008 JAK2, JAK2, PARP, Caspase‐3, Actin (Cell Signaling Technology); SOCS5 (Santa Cruz Biotechnology). Human phospho‐kinase array and human angiogenesis antibody array were performed following manufacturer's instructions (R&D Systems). For phosphor‐kinase array, ∼300 μg HUVEC lysates were analysed 48 h after transfection of control oligo or miR‐9. For human angiogenesis array, MVs were purified from 5 × 106 SK23 cells transfected with scrambled sequence or anti‐miR‐9, and subjected to the antibody array.
Dual luciferase reporter assay
For miR‐9 target validation, 3′ UTR segment of human SOCS5 was cloned into a mammalian expression vector with dual luciferase reporter system (GeneCopoeia). COS‐7 cells were transfected in six‐well plates using Lipofectamine 2000 (Invitrogen). Transfections were performed using 1 μg dual luciferase reporter plasmids and a final concentration of 10 nM synthetic miRNA mimics (Applied Biosystems). Forty‐eight hours after transfection, dual luciferase assays were performed using Luc‐Pair miR luciferase assay kit (GeneCopoeia) according to manufacturer's instructions. Firefly luciferase activity was first normalized to Renilla luciferase expression control. For each reporter construct, the normalized value for miR‐9 transfection was then normalized to the value obtained from the same reporter construct co‐transfected with control miRNA. Mean values, standard deviations and Student's t‐test were calculated from seven independent transfections for each condition. The QuikChange II XL site‐directed mutagenesis kit (Agilent) was used to mutate miR‐9 binding sites at SOCS5 3′ UTR.
Tumour models
Tumour cells (1 × 10
6) were subcutaneously implanted in the dorsal flank of BALB/c Nude mice. Anti‐VEGF mAb B‐20.4.1 (
Liang et al, 2006) or anti‐Ragweed control was IP injected at the dose of 10
mg/kg twice weekly. Antagomirs (Exiqon) were mixed with
in vivo‐jetPEI transfection reagent (Polyplus) and injected intratumorally at 2 μg per mouse twice a week. JAK2 inhibitors GNE‐372 (100
mg/kg) or vehicle control (0.5% methylcellulose/0.2% Tween‐80) were administered twice daily by oral gavage. Tumour volumes (10 animals per group) were measured with digital caliper and calculated as length × width
2 × 0.52. To quantify perfused tumour vessels, fluorescein‐labelled lectin (Vector Lab) was injected intravenously (2
mg/kg) 10 min before collecting tumours. All animal protocols were approved by the Genentech animal care and use committee.
Vascular staining and quantification
Tumours from six mice per treatment group were collected and embedded in OCT blocks. Tissues were cryo‐sectioned to 16 μm thickness on Leica CM3050S, and stained with CD31 antibody (BD Biosciences). Images were acquired with Zeiss AxioImager Z1 fluorescence microscope controlled by TissueFAXS software. Image files were loaded into the TissueStudio analysis package (v1.5, Definiens). Necrotic tissues and staining artifacts such as skin tissues and folds were automatically identified and excluded based on nuclei staining. Blood vessel density was calculated as the ratio of CD31‐positive pixels to the total viable tumour area. Statistical analysis was performed in JMP software.
Statistical analysis
Rank products analysis was performed on the miRNA profiling results to identify most significantly changed miRNAs in response to tumour stimulation, and a permutation approach was used to compute the empirical
P‐values (
Breitling et al, 2004). The results were graphed in volcano plot, and miRNAs with
P<0.001 were highlighted. In all experiments, comparisons between two groups were based on two‐sided Student's
t‐test and one‐way analysis of variance (ANOVA) was used to test for differences among more groups.
P‐values of <0.05 were considered statistically significant.
Acknowledgements
We thank the Genentech animal facility, the antibody purification group and the gCell lab. We are grateful to W Ye and D Dornan for their critical reading of our manuscript. We acknowledge X Qu, A Chung, H Tran, R Lesley, B Haley, L Komuves, J Lill, M Nagel and L Lee for their help.
Author contributions: GZ and NF designed the study and wrote the manuscript. GZ, XW, JY, YG, ZM and CB performed the experiments. ZJ and IK provided statistical and imaging analyses, respectively. JO and DS developed the JAK2 inhibitor. All authors contributed to finalise the manuscript.