Hypoxia shifts activity of neuropeptide Y in Ewing sarcoma from growth-inhibitory to growth-promoting effects

Introduction

Ewing sarcoma (ES) is an aggressive malignancy affecting children and adolescents. The presence of metastases is the most adverse prognostic factor, with a 3-year event-free survival at 27% for patients with metastatic tumors [1]. This poor prognosis is associated with a frequent disease recurrence, suggesting that ES tumorigenic potential is driven by chemotherapy-resistant, metastatic cancer stem cells (CSCs). A population of ES cells with elevated aldehyde dehydrogenase (ALDH) activity is particularly rich in CSCs, as shown by its increased tumorigenic potential and chemoresistance [2].

The fraction of CSCs often increases in hypoxia, leading to disease dissemination and resistance to therapy [3-5]. In ES, the hypoxia-driven increase in tumor cell malignancy has been demonstrated using experimental models, while clinically tumor ischemia associates with unfavorable disease phenotype [6-11]. However, the mechanisms governing these effects remain unknown.

Malignant transformation of ES is driven by a chromosomal translocation resulting in fusion of the EWS gene with an ETS transcription factor, most often FLI1 [12]. Neuropeptide Y (NPY) and its Y1R and Y5R are among the transcriptional targets of EWS-FLI, highly expressed in ES tissues and cells [13-18]. However, microarray analysis revealed that mRNA of NPY’s Y2R, which is not detectable in ES cells in vitro, is elevated in tissues from metastatic ES [18, 19]. Given the high release of NPY from many ES cell lines [17], this expression pattern raises a question about the role of the endogenous peptide in these tumors.

NPY is a 36 amino-acid neurotransmitter promoting proliferation and motility of various cells and regulating their differentiation [18, 20-26]. The peptide acts also as an angiogenic factor, stimulating endothelial cells (ECs) via their inducible Y2R [27]. Paradoxically, our data indicate that in ES, the EWS-FLI1-driven Y1R/Y5R/NPY autocrine loop stimulates tumor cell death [17, 18]. However, we have also shown that this effect of endogenous NPY is mitigated by dipeptidyl peptidase IV (DPPIV) expressed in ES cells [17]. This enzyme cleaves full length NPY1-36 to a shorter form, NPY3-36, which does not bind to Y1Rs and is unable to stimulate ES cell death [17, 28]. Importantly, NPY3-36 preserves the ability to activate Y2Rs and Y5Rs and becomes a selective Y2R/Y5R agonist [28]. Thus, given the known role of Y2R in angiogenesis and elevated levels of its mRNA in metastatic ES tissues [19, 29-33], we sought to determine the function of the Y2R pathway in these tumors.

Hypoxia, known to enhance ES malignancy, also regulates the NPY system. As elements of the angiogenic pathway, NPY, its Y2R and DPPIV, which converts the peptide to a Y2R/Y5R agonist, are up-regulated in ischemic tissues [31, 34-36]. Therefore, we hypothesized that Y2Rs, which are undetectable in ES cells in vitro, are induced in the tumor microenvironment by hypoxia. Indeed, we have shown that hypoxic conditions promote NPY-induced angiogenic processes and activate the Y2R/Y5R/DPPIV/NPY3-36 pathway in ES cells, changing the functions of the peptide from growth-inhibitory to growth-promoting activities. The latter is particularly apparent in ALDHhigh CSCs, suggesting a potential role for NPY in promoting the malignant phenotype of hypoxic ES. These findings demonstrate for the first time the dynamic nature of NPY actions in ES and identify mechanisms by which tumor microenvironment converts the peptide to a growth-promoting factor, specific for tumorigenic ES CSCs. Our study also reveals a novel mechanism governing a hypoxia-induced increase in ES malignancy.

Results

Y2R is expressed in endothelium and tumor cells from ES patient biopsies.

Y2R mRNA is elevated in metastatic ES tumors [19]. To identify the specific cells expressing this receptor, tissue sections from 16 human ES tumors were stained with anti-Y2R antibody (Supplementary Table 1). Y2R was present in tumor cells and ECs (Fig. 1A). While ECs uniformly expressed Y2R, the tumors varied in percent of Y2R-positive ES cells, dichotomizing into two groups – low Y2R (0-10% of tumor cells stained) and high Y2R (40-100% of Y2R-positive ES cells) (Fig. 1A). High Y2R expression tended to correlate with worse survival at 23 months post diagnosis (50% and 100% for patients with high and low Y2R, respectively) (Supplementary Fig. 1, Supplementary Table 1). Due to the small sample size, however, the difference did not reach statistical significance (p = 0.09).

In Y2R high tumors, intense Y2R staining was observed around blood lakes, which are perfused pseudovascular structures devoid of endothelial lining and therefore negative for endothelial marker, CD31 (Fig. 1B-E). In ES, such pseudo-vessels are formed by hypoxic tumor cells [10]. Consequently, staining of serial tumor sections revealed that the entire area surrounding blood lakes was positive for a hypoxia marker, CAIX (Fig. 1F) [37]. The cells with the highest CAIX expression were lining the lumens of blood lakes (Fig. 1C, F). The cells demarcating these pseudo-vessels were also highly positive for Y2R (Fig. 1C, E), suggesting preferential expression of this receptor in hypoxic ES cells.

Hypoxia up-regulates the Y2R/Y5R/DPPIV/NPY3-36 system in ES cells.

To determine whether expression of Y2R is induced by hypoxia, ES cells were cultured in 0.1% oxygen, which stabilized Hif-1α within 6h (Fig. 2A). This hypoxic response was associated with changes in the NPY system. Y2R mRNA expression was induced in all ES cell lines tested, while DPPIV mRNA was increased in three out of four cell lines (Fig. 2B). When analyzed as combined changes in all tested ES cell lines, the increases in expression of Y2R and DPPIV were statistically significant, implicating these two genes as universal targets of hypoxia (Fig 2B). Levels of Y1R and Y5R mRNA remained unchanged. Consistently, in SK-ES1 cells, a model of NPY-rich ES [17], Western blot confirmed hypoxia-induced increases in Y2R and DPPIV protein levels, which was associated with elevated activity of the enzyme (Fig. 2C, D). Despite the lack of changes in Y5R mRNA, its protein levels were increased in hypoxic cells, while Y1R remained unchanged (Fig. 2C). Altogether, these hypoxia-induced changes suggested activation of the Y2R/Y5R/DPPIV axis.

Y2R and DPPIV are expressed in hypoxic areas of ES tissue.

To confirm the hypoxia-induced changes in the NPY system in vivo, we used an orthotopic ES xenograft model. Mice bearing SK-ES1 tumors were injected with a hypoxia probe, pimonidazole, and the tumors were harvested 24h later. Staining of tumor tissues with anti-pimonidazole antibody exhibited a characteristic pattern of hypoxic areas located near the necrotic regions, surrounding blood vessels at a distance of approximately 100 µm (Fig. 2E). Double-staining with anti-pimonidazole and anti-Y2R or anti-DPPIV antibody revealed accumulation of both proteins in hypoxic areas (Fig. 2F), supporting observations in human ES tissues (Fig. 1B-F).

Hypoxia prevents the Y1R/Y5R-mediated cell death in ES cells and triggers a stimulatory effect of NPY on their anchorage-independent growth.

NPY stimulates ES cell death via the Y1R/Y5R pathway, while DPPIV counteracts this process by inactivating the peptide at Y1Rs [17, 18]. Since hypoxia up-regulated DPPIV, we sought to determine if this could prevent NPY-induced cell death. In normoxia, the full-length NPY, but not the product of DPPIV cleavage, NPY3-36, decreased the number of SK-ES1 soft agar colonies (Fig. 3A, B). This effect was not observed in hypoxia, the condition favoring DPPIV (Fig. 3A, B). Instead, hypoxia alone increased the size of SK-ES1 colonies, while both NPY and NPY3-36 administered under hypoxic conditions further augmented this effect (Fig. 3A, C). Since anchorage-independent growth depends on CSCs, and NPY3-36 selectively activates Y2R and Y5R, these results suggested a Y2R/Y5R-dependent increase in ES CSC proliferation.

Y2R/Y5R/DPPIV system is preferentially activated in hypoxic ES CSCs.

The results of soft agar assay suggested that hypoxia-induced changes in the NPY system affect CSCs. Thus, in the subsequent experiments, we focused on ES cells with high ALDH activity, which have been shown to be rich in CSCs [2]. Culture under hypoxic conditions increased the number of SK-ES1 cells with elevated ALDH activity (Fig. 4A), suggesting hypoxia-driven enrichment in CSCs. To assess expression of the NPY system in ES CSC, SK-ES1 cells were sorted by flow cytometry into ALDHhigh and ALDHlow cells (Supplementary Fig. 2). This approach allowed for testing two cell populations with maximal difference in ALDH activity. The efficiency of sorting was confirmed by elevated expression of one of the main forms of ALDH, ALDH1, and a stem cell marker, Oct-4, in ALDHhigh cells (Fig. 4B). Western blot analysis of ALDHlow and ALDHhigh cells cultured under normoxic and hypoxic conditions revealed hypoxia-induced up-regulation of Y2R protein in both cell fractions (Fig. 4C). However, in normoxia and hypoxia, expression of DPPIV was higher in ALDHhigh cells, as compared to ALDHlow cells. Consequently, hypoxic CSCs had the highest DPPIV protein and activity levels (Fig. 4C, D).

NPY stimulates proliferation and migration of hypoxic ES CSCs.

Having established hypoxia-induced changes in NPY system expression, we sought to determine their functional consequences. To this end, SK-ES1 cells were sorted into a population of ALDHhigh and ALDHlow cells as above. Although there were no significant differences in basal levels of the proliferation and migration between these cell fractions (data not shown), the cells varied in their responses to NPY.

In normoxia, NPY had no significant effect on the proliferation of ALDHhigh and ALDHlow SK-ES1 cells (Fig. 5A). However, in hypoxia, the peptide selectively stimulated proliferation of ALDHhigh cells. This effect of NPY in hypoxic ALDHhigh cells was mimicked by Y2R/Y5R-specific treatment - the full-length NPY in the presence of Y1R antagonist or a Y2R/Y5R selective agonist, NPY3-36 (Fig. 5A). Consequently, both Y2R and Y5R antagonists reduced the mitogenic effect of NPY in hypoxic ALDHhigh cells (Fig. 5A).

Similar to its proliferative actions, full-length NPY stimulated migration preferentially in hypoxic ADLHhigh SK-ES1 cells (Fig. 5B). Treatment with NPY in the presence of Y1R antagonist or with NPY3-36 further enhanced the NPY-induced SK-ES1 cell migration in hypoxia. This Y2R/Y5R-specific treatment also moderately increased migration of normoxic ALDHhigh and ALDHlow cells (Fig. 5B). The effect of NPY in hypoxic ALDHhigh cells was blocked by the combination of Y2R and Y5R antagonist (Fig. 5B). Altogether, these results demonstrate the Y2R/Y5R-mediated mitogenic and pro-migratory activity of NPY, which is triggered by hypoxia favoring the Y2R/Y5R/DPPIV system in ES CSCs.

Hypoxia enhances the ability of ES cells to stimulate angiogenesis via release of NPY.

NPY is an angiogenic factor acting via its Y2R, the expression of which is induced in ECs by hypoxia or exposure to NPY [27, 31]. The peptide has been previously implicated in the vascularization of ES tumors [18]. To determine if its angiogenic effect is enhanced by hypoxia, we used two ES cell lines varying in NPY release [17]. In SK-ES1 cells, which constitutively express high levels of NPY, 24h culture in hypoxia further increased NPY synthesis and release (Fig. 6A). No increase in NPY expression was observed in ES925 cells, which do not secrete the peptide under basal conditions (Fig. 6A).

To determine functional consequences of these changes, we tested the effect of conditioned media from normoxic and hypoxic ES cells on HMVEC proliferation. The proliferative effects of conditioned media from normoxic SK-ES1 and ES925 were comparable and not dependent on NPY, since Y2R antagonist did not significantly decrease them (Fig. 6B). Conditioned media from hypoxic SK-ES1 cells exerted a higher proliferative effect, as compared to the media from normoxic cells (Fig. 6B). This hypoxia-induced increase in HMVEC proliferation was blocked by Y2R, proving its dependency on NPY. No statistically significant increase in proliferative activity of conditioned media from hypoxic ES925 cells was observed, consistent with the lack of NPY release from these cells (Fig. 6A, B).

Hypoxia sensitizes ECs to NPY released from ES cells.

Having established the hypoxia-induced increase in NPY release from ES cells, we sought to determine if its angiogenic activity can be augmented by parallel changes in ECs. HMVECs were cultured in 0.1% oxygen, which up-regulated Hif-1α within 6h (Fig. 7A). After 24h, hypoxia induced Y2R, which was not detectable in normoxic HMVECs (Fig. 7A). Simultaneously, hypoxia increased DPPIV protein levels (Fig. 7A) and augmented its activity up to 140% of the normoxic control (data not shown). This hypoxia-induced activation of the Y2R/DPPIV system sensitized HMVECs to NPY. The mitogenic activity of the peptide was elevated in hypoxic HMVECs, as compared to the normoxic cells (Fig. 7B). In normoxia and hypoxia, NPY effects were blocked by Y2R antagonist. Similarly, NPY-rich SK-ES1 conditioned media exerted enhanced proliferative activity in hypoxic HMVECs, as compared to normoxic cells (Fig. 7C). Y2R antagonist blocked this effect, thereby confirming its dependency on activation of the Y2R/DPPIV system in ECs. The proliferative activity of ES925 conditioned media, which lacks NPY, was also higher in hypoxic HMVECs (Fig. 7C). However, Y2R antagonist did not block this increase.

Y2R antagonist reduces vascularization of ES xenografts.

Our observations in vitro suggested that the angiogenic activity of NPY in ES is induced in tumor microenvironment by hypoxia. To confirm this, SK-ES1 subcutaneous xenografts were treated with Y2R antagonist. This blockage of Y2R resulted in significant decrease in tumor vascularization, as measured by area of CD31-positive endothelial cells (Fig. 8A, B). This effect was associated with reduced mRNA levels of mouse vascular endothelial growth factor receptor 2 (VEGFR2) (Fig. 8C). Altogether, these results confirm the role of NPY and its Y2R in ES vascularization.

Discussion

Growing evidence indicates a role of hypoxia in ES progression. In ES patients, tumor ischemia is associated with an unfavorable metastatic pattern, while its absence correlates with better prognosis [11]. In vitro, hypoxia up-regulates EWS-FLI1 protein and modifies its transcriptional profile, promoting genes involved in tumor progression [6]. Hypoxic ES cells exhibit an enhanced anchorage-independent growth, invasiveness, and resistance to apoptosis induced by exogenous factors [6-9, 38]. However, the mechanisms of these effects remain unclear. In fact, some data indicate no hypoxia-induced changes in ES cell proliferation, but rather an increase in apoptosis when the cells are assayed as a whole population in adherent culture [6, 7]. Thus, such a hypoxia-induced increase in tumor malignancy may be driven by specific changes in CSCs.

CSCs are resistant to low oxygen and their fraction increases in hypoxia-treated tumor cells [3-5]. In our study, hypoxic conditions increased the population of ES cells with high ALDH activity, which are rich in tumorigenic CSCs. We propose that this enrichment in ES CSCs in combination with activation of the Y2R/Y5R/DPPIV/NPY3-36 system in these cells is one of the driving mechanisms governing the hypoxia-driven increase in ES malignancy.

NPY, and its Y1R and Y5R are transcriptional targets of EWS-FLI1 up-regulated in ES [13, 14]. Paradoxically, we have previously shown that this Y1R/Y5R/NPY autocrine loop stimulates ES cell death [17, 18]. However, mRNA of another NPY receptor, Y2R, is up-regulated in metastatic ES tissues [19]. Since Y2R is not detectable in cultured ES cells [18], the goal of our study was to determine its localization and function in ES. Y2R was present in ECs, but also in tumor cells, and observed to accumulate in hypoxic areas. Consistently, we have shown that Y2R expression is induced in ES cells by hypoxia. This effect was associated with increases in NPY release, Y5R protein levels, and in expression of DPPIV, an enzyme converting the peptide to a selective Y2R/Y5R agonist. These changes suggested an overall hypoxia-induced activation of the Y2R/Y5R/DPPIV/NPY3-36 axis. Similar up-regulation of the NPY system was reported in ischemic tissues, while DPPIV was elevated in various hypoxic tumor cells [31, 34-36].

ES cells are rich in Y1R, which is expressed in response to EWS-FLI1 [13-16, 18]. However, in hypoxia, Y1R expression did not change, while levels of Y2R and Y5R increased, altering the NPY receptor ratio. Moreover, increased DPPIV activity, such as that observed in hypoxic ES cells, alters the form of released NPY to NPY3-36, a selective Y2R/Y5R agonist [17]. Altogether, these changes prevent binding of NPY to Y1Rs and block ES cell death mediated by the Y1R/Y5R/NPY1-36 pathway. Furthermore, DPPIV-induced cleavage of NPY enables the activation of moderately expressed Y2Rs and Y5Rs in the presence of abundant Y1Rs. We have shown that while Y2Rs are induced in both ALDHhigh and ALDHlow, DPPIV is preferentially up-regulated in ALDHhigh cells. Our results are in agreement with reports of DPPIV serving as a marker of metastatic CSCs in other tumors [39].

Consistent with preferential DPPIV activation in CSCs, NPY stimulated the proliferation of hypoxic ALDHhigh cells, but not ALDHlow cells. The fact that either Y2R or Y5R alone blocked this effect suggested that activation of both receptors is required to trigger it. The selective mitogenic activity of NPY in ALDHhigh cells is consistent with reports indicating differential effects of hypoxia and NPY on ES cells, depending on culture conditions. While both factors increase the size of CSC-dependent soft agar colonies, they have no effect on the proliferation of non-sorted, adherent cells, comprised mostly of non-CSCs [6, 7, 18].

As observed for its proliferative effect, full-length NPY stimulated migration only in hypoxic ALDHhigh cells. However, treatment with NPY in the presence of Y1R antagonist or with NPY3-36 alone augmented this effect and moderately increased cell migration in normoxic ALDHhigh and ALDHlow cells. These observations suggest that in normoxia, selective activation of Y5Rs is sufficient to stimulate ES cell migration, while hypoxia-induced expression of Y2Rs further augments this process. Consequently, both Y2R and Y5R antagonists were required to block the pro-migratory effects of NPY in hypoxic ALDHhigh cells, suggesting that independent activation of one of these receptors promotes cell migration. Altogether, our data indicate that hypoxia-induced changes in NPY functions are particularly apparent in a CSC-rich ALDHhigh cells. These changes may contribute to the increase in ES metastatic properties, albeit without an effect on the primary tumor growth that is dependent mostly on non-CSCs. Future studies with animal models will explore this hypothesis.

The angiogenic activity of NPY depends on Y2R [30]. In hypoxic NPY-rich ES cells, simultaneous increases in NPY and DPPIV expression led to elevated release of the peptide, presumably as a Y2R/Y5R-selective agonist, NPY3-36. This, in turn, increased the angiogenic activity of ES conditioned media. This stimulatory effect was further enhanced by increases in Y2R and DPPIV expression in hypoxic ECs, which sensitized them to NPY’s proliferative effect. Consequently, Y2R antagonist significantly reduced vascularization of NPY-rich ES xenografts. Y2R expression in ECs within human ES tissues supported the clinical relevance of these findings.

The elevated responsiveness of hypoxic ECs to ES conditioned media lacking NPY implicated a role for other ES-derived angiogenic factors, such as VEGF [40]. Importantly, the NPY and VEGF angiogenic systems are interdependent, with NPY serving as an upstream factor [31, 41]. Consistently, Y2R antagonist decreased expression of VEGFR2 in NPY-rich SK-ES1 xenografts, suggesting that VEGF pathway activation is NPY-dependent. Importantly, SK-ES1 cells have low basal VEGF levels and lack mechanisms that mediate its hypoxia-induced up-regulation in other ES cells [40]. Therefore, in the subset of such VEGF-insufficient tumors, hypoxia-induced activation of the NPY system is essential to maintain tumor vascularization by direct stimulation of ECs and up-regulation of VEGF system.

NPY receptor patterns in ES and ECs are similar, with constitutively expressed Y1R and inducible Y2R [17, 27]. Consequently, in both cases, DPPIV-induced NPY cleavage is essential to enable activation of Y2Rs, which are expressed at lower levels than abundant Y1Rs. These observations suggest a potential for multifunctional therapies for ES. Since the same Y2R/Y5R/DPPIV/NPY3-36 system is responsible for hypoxia-induced proliferative and pro-migratory effects of NPY in ECs and ES CSCs, blocking this pathway in vivo may target both metastatic and angiogenic properties of the tumors. This has been shown in neuroblastoma, where Y2R antagonist reduced xenograft growth via inhibition of tumor cell proliferation and vascularization [27].

In addition to the typical vasculature, ES tumors are known to form pseudo-vessels, also called blood lakes, which augment blood flow to the tumor tissue. An increased presence of these structures is associated with poor prognosis in ES patients [42]. The formation of pseudo-vessels is driven by hypoxia [10]. Consistently, the tumor cells surrounding them are positive for hypoxia markers, as well as Y2R. These observations warrant further investigation as to the potential role for Y2R and NPY in vascular mimicry.

Altogether, our results revealed the dynamic nature of NPY actions in ES and critical role of the tumor microenvironment in their regulation. The net effect of endogenous NPY on ES depends on the balance between Y1R/Y5R/NPY1-36 growth-inhibitory effects on the entire population of ES cells and Y2R/Y5R/DPPIV/NPY3-36 proliferative and pro-migratory effects on ES CSCs and ECs (Fig. 9). Hypoxia shifts this balance toward growth-promoting processes by preventing activation of Y1Rs and promoting the Y2R/Y5R pathway. Further studies are required to determine the impact of these changes in the NPY system on ES progression and metastases.

Despite the complexity of NPY functions in ES, the receptor specificity of its actions and potential for multifaceted therapeutic effects make the peptide and its receptors attractive targets in ES treatment. We have shown that exogenous NPY inhibits ES xenograft growth via Y1R/Y5R-mediated cell death [17, 18]. Thus, receptor specific interventions activating the Y1R/Y5R pathway, inhibiting Y2R/Y5Rs, and/or targeting DPPIV may provide new therapeutic opportunities for ES patients. Recently, a variety of selective NPY receptor agonists and antagonists have been developed. This includes Y1R/Y5R selective agonists and various Y2R antagonists [43]. Some of them, such as DPP inhibitors and Y5R antagonist are already being used in clinical practice or trials for other disorders [44-46]. Importantly, however, our previous studies indicate that prolonged treatment of ES xenografts with DPP inhibitors results in increased DPPIV expression, which overcomes their effects [17]. While this could possibly be circumvented by changes in drug regimen or its potency, targeting NPY receptors may be a better therapeutic strategy. This approach is also more specific, given the high range of known DPPIV substrates.

In summary, we have shown for the first time fundamental changes that can occur in the NPY/DPPIV system within the tumor microenvironment and their functional consequences. Our findings highlight the importance of assessing NPY functions in tissue environment, uncover its novel role in cancer stem cells and reveal mechanisms governing a hypoxia-induced increase in tumor malignancy. Although our study focuses on ES, hypoxia-induced activation of the Y2R/Y5R/ DPPIV/NPY3-36 axis may be applicable to other tumors rich in NPY and its receptors. A similar pattern of NPY receptor expression and its effect on tumor cell proliferation and migration has been reported in breast cancer [21, 23]. The evidence of a role for both NPY and DPPIV in a variety of other tumors is also growing [18, 27, 47-49]. Thus, understanding the NPY system may direct new therapeutic opportunities for patients with metastatic ES, thus far lacking an effective treatment, as well as those with other malignancies.

Methods

Materials:

NPY and NPY3-36 were purchased from Bachem (San Carlos, CA); Y1R antagonist, BIBP 3226, from Sigma (St. Louis, MO); Y5R antagonist, CGP71683, and Y2R antagonist, BIIE0246, from Tocris (Ellisville, MO). DPPIV inhibitor, Sitagliptin, was a gift from Dr. Bachovchin (Tufts University, Boston, MA).

Human tissue sections from 16 ES archival paraffin embedded samples were collected from multiple institutions in Poland by one of the co-authors (EIS) in compliance with institutional ethical regulations. Use of these samples was approved by Georgetown University Institutional Review Board.

ES xenografts:

For the orthotopic xenografts, SK-ES1 cells were injected into gastrocnemius muscles of SCID/bg mice [50]. Once tumors reached 1cm3, mice were injected intraperitoneally with a hypoxia probe, pimonidazole (HPI, Burlington, MA), 1.5mg/mouse, and tumors were harvested 24h later. For the subcutaneous xenografts, SK-ES1 cells were injected into nude mice and treated daily with local injections of Y2R antagonist (10-6M) [17, 27]. Treatment was initiated when the tumors reached a volume of approximately 100mm3, and the experiment was terminated 2 weeks later. Tumor vascularization was quantified by immunohistochemistry, as area of positive staining for endothelial marker, CD31, while expression of mouse vascular endothelial growth factor receptor 2 (VEGFR2) was measured by real-time RT-PCR.

Immunohistochemistry

Immunohistochemistry was performed using the following antibodies: rabbit polyclonal anti-Y2R (Neuromics, Edina, MN), anti-CD26 (Novus Biologicals, LLC, Littleton, CO), anti-pimonidazole (HydroxyprobeTM-1 kit) (HPI, Inc. Burlington, MA), anti-carbonic anhydrase IX (CAIX) and anti-mouse CD31 (Abcam, Cambridge, MA) and mouse monoclonal anti-human CD31 (DAKO, Carpinteria, CA). Staining intensity was quantified using Metamorph software.

Cell culture:

Human ES cells were obtained and cultured as previously reported [17]. Human dermal microvascular endothelial cells (HMVEC) purchased from Lonza (Basel, Switzerland) were cultured according to the supplier’s recommendation. Hypoxia was created in a chamber containing 0.1% O2, 95% N2 and 5% CO2.

Real time RT-PCR and NPY ELISA were performed as previously described [17, 18].

Aldefluor assay and cell sorting:

ES cells were stained using ALDEFLUOR kit (Stemcell Technologies, Vancouver, Canada). Fluorescence-activated cell sorting (FACS) was performed on FACSAria (BD, Franklin Lakes, NJ) utilizing FACSDiva and FCS Express 4 softwares (DeNovo Software, Los Angeles, CA). Cells were sorted into ALDHhigh (upper 8%) and ALDHlow cells (lower 10%), cultured for no longer than 24h in normoxia or hypoxia, and assayed as desired. ALDH activity in normoxia and hypoxia was measured by FACS upon 24h culture.

Cell membrane isolation and Western blot:

Cell lysates were fractionated into membrane and soluble proteins, as previously described [51]. Western blot was performed using the following antibodies: rabbit polyclonal anti-Y1R (gift from Dr. Urban, University of Chicago), anti-DPPIV and anti-CAIX (Abcam, Cambridge, MA), anti-flotilllin-1 (Sigma, St. Louis, MO) and anti-hypoxia-inducible factor 1α (Hif-1α) (Cell Signaling Technologies, Danvers, MA), goat polyclonal anti-Npy2r (My Biosource, Camarillo, CA) and anti-Y5R (Everest Biotech, Ramona, CA) and mouse monoclonal anti-ALDH1 (BD Biosciences, San Jose, CA), anti-Oct-4 (Santa Cruz Biotechnology, Santa Cruz, CA) and anti-β-actin (Sigma, St. Louis, MO).

DPP activity from unsorted cells was measured calorimetrically, as previously described [17], while for sorted ES cells DPPIV-Glo™ Protease Assay (Promega, Madison, WI) was used. DPPIV activity was calculated as a fraction of DPP activity blocked by its selective inhibitor, Sitagliptin (10-5M) [17].

Colony formation on soft agar was performed as previously described [17]. Cells were treated with NPY or NPY3-36 (10-7M) and incubated in normoxia or hypoxia for 14 days.

ES cell proliferation was measured using Click-iT® EdU cell proliferation assay (Life Technologies, Grand Island, NY). ALDHhigh and ALDHlow ES cells were pre-incubated in normoxia or hypoxia for 6h and treated with NPY (10-7M) +/- receptor antagonists (10-6M) or with NPY3-36 (10-7M) for 12h. Cells were pulsed with EdU, fixed and fluorescently labeled according to the manufacturer’s procedure. Proliferation was measured as a percent of EdU-positive cells.

ES cell migration:

ALDHhigh and ALDHlow cells were plated onto BD FluoroBlok™ 96-well plates (BD Biosciences, San Jose, CA), pre-incubated for 6h in hypoxia or normoxia and treated as above for 18h. Cells were stained with Calcein AM and fluorescence was measured from the bottom of the plate.

HMVEC proliferation:

ES cells were grown in HMVEC culture media, which was collected 24h later. HMVECs were plated onto 96-well plates, growth-arrested for 24h, and then treated for 24h with NPY (10-8M) or ES-conditioned media, +/- Y2R antagonist (10-6M). Proliferation was measured using [3H] thymidine [18].

Statistical analysis:

Statistical analysis was performed using SigmaStat® and GraphPad softwares. One-way repeated measure ANOVA with post-hoc t-test (P<0.05) using Dunnett’s method was used for data comparison and analysis. All experiments were repeated at least three times. Data is presented as mean ± standard errors.

Conflict of interest:

The authors declare no conflict of interest.

Acknowledgments:

The authors thank Dr. Aykut Üren for critical reading of the manuscript. This work was supported by National Institutes of Health grants: UL1TR000101 (previously UL1RR031975) from the National Center for Advancing Translational Sciences (NCATS), through the Clinical and Translational Science Awards Program (CTSA), 1RO1CA123211 and 1R03CA178809 to J. Kitlinska and 1RO1CA138212 and 1RO1CA133662 to J. Toretsky, as well as funding from Children’s Cancer Foundation (Baltimore, MD) to J. Kitlinska, Burroughs-Wellcome Foundation Clinical Scientist Award to J. Toretsky and Georgetown Undergraduate Research Opportunities Program to M. Horton and D. Christian. The experiments were performed with use of Lombardi Comprehensive Cancer Center Shared Resources (The Flow Cytometry & Cell Sorting, Histopathology & Tissue, The Biostatistics & Bioinformatics, Microscopy & Imaging and The Tissue Culture Shared Resources) partially supported by NIH/NCI grant P30-CA051008.

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