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. Author manuscript; available in PMC: 2014 Sep 1.
Published in final edited form as: J Invest Dermatol. 2013 Sep 13;134(3):801–808. doi: 10.1038/jid.2013.395

EPIDERMAL DELETION OF HIF-2α STIMULATES WOUND CLOSURE

Andrew S Cowburn 1,3, Laura E Crotty Alexander 4, Mark Southwood 1, Victor Nizet 2, Edwin R Chilvers 1, Randall S Johnson 3
PMCID: PMC3877686  NIHMSID: NIHMS523457  EMSID: EMS54756  PMID: 24037341

Abstract

Wound closure requires a complex series of micro-environmentally influenced events. A key aspect of wound closure is the migration of keratinocytes across the open wound. It has been found previously that the response to hypoxia via the HIF-1α transcription factor is a key feature of wound closure. The need for hypoxic response is likely due to interrupted wound vasculature as well as infection, and in this work, we investigated the need for a highly related hypoxic response transcription factor, HIF-2α. This factor was deleted tissue-specifically in mice, and the resulting mice were found to have an accelerated rate of wound closure. This is correlated with a reduced bacterial load and inflammatory response in these mice. This indicates that manipulating or reducing the HIF-2α response in keratinocytes could be a useful means to accelerate wound healing and tissue repair.

Introduction

Many processes supporting oxygen homeostasis are mediated by a small group of transcriptionally active hypoxia-inducible factors (HIFs). These transcription factors are considered to be the major coordinators of the cellular and systemic responses to hypoxia. HIF is a heterodimer composed of an oxygen-regulated HIF-α subunit (HIF-1α, HIF-2α or HIF-3α) and the ubiquitous aryl hydrocarbon receptor nuclear translocator (HIF-1β). Under normoxic conditions HIF-α protein turnover is generally very rapid due to the action of a set of prolyl hydroxylases; these oxygen-dependent enzymes hydroxylate two proline residues on the HIF-α subunit (Pro402 and Pro564), which promotes binding of the Von Hippel-Lindau (VHL) protein and subsequent targeting of HIF-α for poly-ubiquitination and proteasomal degradation. Despite its close proximity to an oxygen rich ambient environment, the skin is well recognized to be constitutively hypoxic even under normal conditions(Bedogni et al., 2005; Stewart et al., 1982; Varghese et al., 1986), resulting in a degree of constitutive HIF-1α stability in the basal epidermal layer.

In recent years the importance of HIF-1α in wound healing has gained notoriety, with a number of groups demonstrating the role of this transcription factor in the cascade of events leading to wound closure. Following acute injury, the wound area becomes increasingly hypoxic due to loss of vascular structure and the heightened oxygen consumption accompanying the inflammatory response.(Varghese et al., 1986) This hypoxic microenvironment further enhances HIF-1α stability and promotes the release of a number of angiogenic factors (VEGF, FGF-2, PIGF, ANGPT)(Asahara et al., 1999; Grunewald et al., 2006; Rehman et al., 2003; Yoder et al., 2007) that regulate endothelial survival, migration and proliferation, and the formation of new capillaries. Stabilization of dermal HIF-1α also increases the recruitment of circulating endothelial cell precursors to the wound site, which further improves wound revascularization and healing(Ceradini et al., 2004; Jin et al., 2006; Loh et al., 2009). The role of HIF-1α in wound healing derives from a number of studies focused on the effects of depleting HIF-1α. Hence in heterozygous HIF-1α knockout mice the recruitment of endothelial cells is impaired and wound closure delayed.(Zhang et al., 2010)

Reduced levels of HIF-1α protein have been documented in a number of chronic conditions associated with impaired wound healing, including diabetes and aging(Botusan et al., 2008; Loh et al., 2009). HIF-1α enhances the mobility of keratinocytes and dermal fibroblasts through its influence on MMP and integrin expression (Decline and Rousselle, 2001; Deonarine et al., 2007). Furthermore, HIF-1α increases the expression of laminin-332 and subsequent interaction with its receptors integrin-α3β1 and α6β4, activating a signaling cascade to promote cell proliferation, survival and migration.(Decline and Rousselle, 2001; Deonarine et al., 2007; Fitsialos et al., 2008; Iyer et al., 2005; Keely et al., 2009)

In contrast, a potential role for HIF-2α in wound closure remains undefined. While the two HIFα isoforms share a highly conserved amino acid sequence and structure, and are both stabilized under hypoxia and purported to bind the same HRE site, these isoforms appear to have distinct physiological roles. A differential function of HIF-1α and HIF-2α is supported by studies showing non-concordant expression and stability of these isoforms within different cell types and tissues. For example, HIF-1α is stabilized for sustained periods in the brain even following moderate hypoxia, compared to the liver and kidney, where HIF-1α stabilization requires more severe oxygen depletion, and is only transient.(Stroka et al., 2001) In contrast, HIF-2α is stabilized very readily in the liver, but only weakly in the kidney and the brain, and its expression tends to be maintained for much longer time periods.(Wiesener et al., 2003) These observations show clear differences between HIF-1α and HIF-2α, as supported by evidence indicating that HIF-1α and HIF-2α can act in a divergent manner to regulate a range of responses in vivo. Such counter-regulatory roles include functionally opposing interactions with the Myc transcription factors(Florczyk et al., 2011; Gordan et al., 2007) and with the tumor suppressors p53(Bertout et al., 2009) and mTOR.(Toschi et al., 2008) In addition, we have shown that NO homeostasis in macrophages can be differentially regulated through the opposing actions of Th1 and Th2 cytokines on the transcription of HIF-1α and HIF-2α.(Takeda et al., 2010)

To address whether the differential expression of HIF-1/2α isoforms in keratinocytes might affect the physiological process of wound closure, we have used a murine model of HIF-2α knockout targeted to keratinocytes (K14cre-HIF2α animals). These mice have normal HIF-1α expression and normal dermal structure, but demonstrate accelerated wound closure. We have also used a different murine model to heightened HIF-1α stability, the K14cre-VHL/HIF-2α mouse, where deletion of both VHL and HIF-2α from keratinocytes leaves the HIF-1α isoform constitutively stable. This model again results in substantially accelerated wound closure, which is most evident during the initial healing phase.

Results

Keratinocyte migration is accelerated by hypoxia

The migration of human keratinocytes is a critical factor underlying efficient and rapid wound healing. Previous studies have reported the ability of hypoxia to stabilize HIF-1α in the human keratinocyte cell line, HaCaT,(Fitsialos et al., 2008) and the expression of HIF-1α at the leading edge of the wound margin in murine models. The HIF-1α target laminin-332 and its interaction with integrins α3β1 and α6β4 has also been linked to increased keratinocyte migration(Fitsialos et al., 2008). In our initial experiments, we confirmed the influence of hypoxia on keratinocyte migration. HaCaT cells cultured under hypoxia (1% O2) for 16 h resulted in a significant increase in keratinocyte mobility compared to normoxic culture conditions (21% O2) (Figure 1a). We were also able to show that HaCaT cells express HIF-2α in addition to HIF-1α and the ability of hypoxia to enhance HIF-2α stability (Figure 1b).

Figure 1. Hypoxia increases the speed of migrating keratinocytes.

Figure 1

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HaCaT cells were grown to 85% confluence prior to undertaking a scratch assay under normoxic (21%) and hypoxic (2% oxygen). (a) The scratch area was calculated from a digital image taken initially and 16h post culture. Data shown as the scratch area as a percentage of control (n=8, *p<0.05). Photomicrographs show representative keratinocyte migration speeds. (b) Representative Western blot showing the stability of HIF-1α and HIF-2α in the keratinocyte cell line HaCaT following exposure to hypoxia (2% oxygen). Cells were harvested at 0, 1, 3, 6, 12 and 24h post hypoxia. (c) Wounds from wild-type mice (n=4) were harvested at days 1, 3, 5, 7, lysed and Western blotted for HIF-1α and HIF-2α protein stability. The bar graph shows the ratio of HIF-α against β-actin (au ± SEM) control with a representative Western blot below.

Inflammatory responses during wound closure

The sequence of cellular events that follows experimental skin wounding is well documented. Several studies have documented the time-course of the ensuing inflammatory cell infiltrate, and the subsequent expression of anti-microbial peptides, nitric oxide synthase 1-3 (NOS1-3) and arginase-1/-2 in the wound margin during the closure period. We wished to confirm these findings in wild-type (WT) mice and compare to changes observed in the K14cre-HIF2α mouse. We performed 8 mm circular full thickness punch biopsies on the back skin of 10-12 week old wild-type mice; wounds were harvested at days 1-13. Bacterial counts (CFU) within the wound margin, including members of the normal skin microflora, were assessed by dilution plating on Todd-Hewitt broth agar plates. Bacterial colonization of the wound area was observed during the acute inflammatory phase (days 1-3) and thereafter the number of CFU diminished until day 5 when the wound area exhibited a full sanguineous crust (Figure 2a). This crust forms a protective barrier that is subsequently re-colonized in association with a second CFU peak at day 10. The crust then recedes, paralleled with a reduction in the CFU counts, with normal flora colonization restored by day 13.

Figure 2. Characterization of environmental bacterial flora and inflammatory response genes during wound closure.

Figure 2

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(a) Wounds were harvested from wild type mice throughout the closure period and bacterial flora (CFU/mg protein) determined. Photomicrographs above the graphic show the general state of the wounds at the time in days shown. Photomicrograph to the right of the graphic shows a representative bacterial culture plate at day 1. (b, c, d, e) QPCR analysis (fold change) of primers for MPO, F4/80, CRAMP, NOS1-3, and arginase-1 and 2 from wild type wounds during the experimental period.

Inflammatory cell infiltration into the wound area was determined by using specific qPCR primers for MPO and F4/80 (Figure 2b) antimicrobial cathelicidin, CRAMP (Figure 2c), NOS1-3 (Figure 2d) and arginase-1/-2 expression (Figure 2e). These data confirm previous observations of an initial rapid inflammatory cell infiltration on day 1-3 followed by a prolonged, lower magnitude macrophage response (days 1-7). The expression of CRAMP parallels very closely the MPO signal, suggesting that it may be principally neutrophil-derived. NOS-2 also increased rapidly in the open wound, then slowly decreased as the wounds closed, returning to near normal expression by day 13; by contrast, NOS-1 and NOS-3 expression was relatively stable throughout the closure period. Arginase-1 and-2 were increased in the wound margin from days 2-9, possibly reflecting their role in collagen deposition.

HIF-α stability in the wound margin during closure

It is well established that mouse skin is hypoxic even under physiological conditions, and previous groups have shown HIF-1α stability at the wound margin. Consequently we determined the stability profile for both HIFα isoforms during the initial 7-day period post wounding. Full thickness dermal wounds were harvested from 4 wild-type mice at days 1, 3, 5, and 7 post-wounding and the expression of HIFα isoforms determined by western blotting. As anticipated, HIF-1α expression increased over the closure period before plateauing at days 5 and 7. We also demonstrated an increase in HIF-2α stability on days 1, 3 and 7, with a significant increase in expression by day 5 (Figure 1c). Previous studies have also documented the expression profiles of HIF-α target genes, arginase-1/-2, and NOS2 over the wound closure period. We further analyzed the wound samples (Supplementary Figure 1 online) and show enhanced expression of both arginase-2 and NOS2 across the wound closure time course with little change in NOS3 expression.

Wound closure is accelerated in the K14cre-HIF-2α mice

To address the in vivo role of HIF-2α in the physiology of wound closure, we next generated mice in which HIF-2α deficiency was restricted to keratinocytes by crossing mice homozygous for the floxed HIF-2α allele with mice expressing Cre recombinase under the control of the keratinocyte promoter (K14cre). Adult K14cre-HIF-2α and WT male mice (10-12 weeks old) received an 8 mm full thickness dermal punch biopsy on the back. Wound closure was measured digitally over the next 10-days. We found wound closure speed to be significantly increased in the K14cre-HIF-2α mice compared to age-matched WT mice (n=12); this was most evident at days 3-6 with the wound closure speed converging to match the normal WT by day 7 (Figure 3a) (n=15). Analysis of keratinocyte migration at the wound margin was determined by calculating the leading edge ratio, i.e. the distance covered by the keratinocyte leading edge divided by the overall wound margin. This ratio was significantly greater in the K14cre-HIF-2α mice (n=6) when compared to WT control (n=6) (Figure 3b-c). High magnification photomicrographs of H&E stained wound margins from WT and K14cre-HIF2α mice showed significantly greater keratinocyte motility in the HIF-2α mutants (Figure 3d). The enhanced keratinocyte motility may be linked to altered expression/activity of c-myc and its overall influence of cell cycle progression. Given that a number of recent publications have described the opposing roles of HIF-1α and HIF-2α on c-myc activity, we proceeded to analyze the expression of a number of c-myc targets (Supplemental figure 2). Keratinocyte deletion of HIF-2α significantly reduced the expression of CDKN1a and influenced a reduction in CDKN1b and E2F1 expression when compared to wild-type control

Figure 3. K14cre-HIF-2α mice show a faster wound closure and keratinocyte migration speed.

Figure 3

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(a) Digital images of wounds from K14cre-HIF-2α (n=12) and wild-type (n=15) were analyzed daily throughout the closure period. The data are presented as percentage wound closure compared to the original wound size (*p<0.05). (b and c) Keratinocyte leading edge analysis. Digital images of H&E stained wounds were captured using a Leica scope and software. The distance of keratinocyte migration divided by the total distance of the wound margin gave a leading edge ratio (leading edge ration=(a+b)/c). The keratinocyte leading edge from the K14cre-HIF-2α wound margin (n=6) was significantly greater than in the wild type controls (n=6) (*p<0.05). (d) High magnification of H&E stained wounds from wild type and K14cre-HIF-2α mice taken on days 1 and 5. Yellow lines outline the migrating keratinocyte leading edge.

Reduced acute inflammatory responses in K14cre-HIF-2α mice

Having previously described the importance of keratinocyte HIF-1α in the transcriptional regulation of two anti-microbial factors, cathelicidin and NO, we proceeded to analyze the wounds from the K14cre-HIF-2α mice for bacterial counts (colony-forming units = CFU) during the initial inflammatory phase (days 1-3) (Figure 4a). Curiously, deletion of epidermal HIF-2α lowered recovered CFU by at least 1-log order on days 1-2 when compared with WT control mice (Figure 4a). Furthermore, qPCR analysis for MPO expression in the wound margin was also significantly lower in K14cre-HIF-2α mice on day 2 (Figure 4b), consistent with reduced neutrophil recruitment and inflammatory response. The expression profile for CRAMP (Figure 4c) matched that for MPO, with a significant reduction in the HIF-2α mutant mice. However, little change was noted in expression for NOS1-3 (Figure 4d) between K14cre-HIF-2α mice and WT controls.

Figure 4. K14cre-HIF-2α mice show reduced wound environmental bacterial flora and reduced acute inflammatory responses.

Figure 4

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(a) Bacterial flora (CFU/mg tissue) were calculated from the wounds of K14cre-HIF-2α (n=4) and wild type control (n=4) during the initial 3 days post wounding, and compared to normal background bacterial flora (control). (b and c) QPCR analysis (fold change) of primers for MPO, F4/80 and CRAMP showed a significantly reduced signal in the wounds from K14cre-HIF-2α (n=4) on day 2 when compared to wild type control (n=4) (d) QPCR analysis (fold change) of NOS1-3 showed little deviation between K14cre-HIF-2α (n=4) and wild type controls (n=4).

Epidermal deletion of VHL and HIF-2α increases wound closure

As a key regulator of HIFα protein stability, the effects of deleting the tumor suppressor VHL were examined in combination with HIF-2α deletion, by generating a K14cre-VHL/HIF-2α mouse. As anticipated, the resultant increase in keratinocyte HIF-1α expression (Supplemental figure 3) in these mice greatly increased wound closure between days 1-5 (Figure 5a). The exaggerated wound closure is depicted in the photomicrographs taken from WT vs. K14cre-VHL/HIF2α mice between days 1-9 (Figure 5b). Detailed analysis of wound samples during the initial 3 days (acute inflammatory phase) showed bacterial counts to be significantly lower on days 1 and 2 post-wounding.

Figure 5. K14cre-VHL/HIF-2α mice show faster wound closure between days 1-5.

Figure 5

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(a) Digital images of wounds from K14cre-VHL/HIF-2α (n=8) and wild-type (n=12) were analyzed daily throughout the closure period. The data are presented as percentage wound closure compared to the original wound size (*p<0.05). Digital photomicrographs show representative images of wound closure from days 1-9 for wild type and K14cre-VHL/HIF-2α. (b) Bacterial flora (CFU/mg tissue) were calculated from the wounds of K14cre-VHL/HIF-2α (n=3) and wild type control (n=4) during the initial 3 days post wounding. (c and d) QPCR analysis (fold change) of primers for CRAMP and MPO, F4/80 showed a significantly reduced signal in the wounds from K14cre-VHL/HIF-2α (n=3) on day 1 when compared to wild type control (n=4) (e) QPCR analysis (fold change) of NOS1-3 showed little deviation between K14cre-VHL/HIF-2α (n=3) and wild type control (n=4).

The marginal increase in CRAMP and MPO expression in the K14cre-VHL/HIF-2α mice at baseline could in part account for the lower initial bacterial counts. Fewer bacteria would be predicted to result in a reduced acute inflammatory response, perhaps reflected in a lower MPO and CRAMP response on day 1 post-wounding compared to WT controls. Although we suggest the acute inflammatory response in the open wound is potentially lower in the K14cre-VHL/HIF-2α mice, the expression of NOS1 and-3 in the mutant mice were not different from WT controls and NOS2 trended towards a higher expression on days 2 and 3 post-wounding.

Discussion

There is a great deal of experimental evidence suggesting that the initial heightened hypoxic environment within an open wound is pivotal in promoting tissue repair, in part through increasing the stability of HIF-1α(Tandara and Mustoe, 2004). The purpose of this study was to assess for the first time the involvement of HIF-2α in wound closure using an in vivo conditional keratinocyte knockout model. The results of this study show that HIF-2α is stabilized in the wound margin from day 1 through to day 7, and that K14cre-HIF2α mice lacking keratinocyte HIF2α expression show: (i) significantly increased wound closure speed at early time points, (ii) increased keratinocyte migration at the leading edge of the wound, and (iii) reduced bacterial load in the open wound during the initial acute inflammatory phase. These striking effects of keratinocyte HIF-2α deletion were accentuated when VHL was coordinately deleted (Figure 5). This manuscript therefore reveals opposing roles for keratinocyte HIF-2α when compared to the established role of HIF-1α in wound healing.

The contrasting roles of HIF-1α and HIF-2α become all the more pertinent when consideration is given to the interactions of HIF-α with Myc transcription factors(Gordan et al., 2007). HIF-2α is known to augment c-Myc activity through the stabilization of c-Myc:Max complex, which promotes cell cycle progression; in contrast HIF-1α inhibits the function of c-Myc resulting in cell cycle arrest. Hence Waikel and colleagues(Waikel et al., 2001) have shown that targeted over-expression of c-Myc in epidermal stem cells (K14) results in the loss of hair follicles and the spontaneous development of ulcerated lesions due to severely impaired wound closure. There model demonstrated a severe depletion in the number of epidermal stem cells and a significant impairment of keratinocyte migration. Therefore in our keratinocyte model, deleting HIF-2α will enable HIF-1α to function unopposed, reducing the activity of c-myc and subsequently increase keratinocyte migration at the leading edge.

Previously we have shown a central role for HIF-1α in the production of cathelilcidin antimicrobial peptides within the epidermis. In the normal or physiologically hypoxic environment of the skin, epidermal deletion of HIF-1α dramatically increased the susceptibility of the skin to infection with group-A Streptococcus(Peyssonnaux et al., 2008). In addition, pharmacological stabilization of HIF-1α limits S. aureus proliferation and lesion formation in a mouse skin abscess model(Okumura et al., 2012). The majority of dermal wounds are colonized with aerobic and anaerobic bacteria and the density and type of these bacterial are important in predicting wound closure speed(Bowler et al., 2001). The mice for this study were individually housed in a clean facility to reduce cross contamination and prevent the introduction of hostile pathogens. In this paper we demonstrate reduced environmental bacterial counts on the skin of K14cre-HIF2α mice, which remained significantly suppressed throughout the acute inflammatory phase of wound closure (days 1-3). This observation was further accentuated in the K14cre-VHL/HIF-2α mice with environmental bacterial counts significantly lower across all time periods studied. Surgical aseptic practice aims to reduce bacterial load on the skin with the intent of lowering the intensity and duration of the inflammatory phase and to increase wound closure speed. The administration of prophylactic antibiotics has also been show to significantly reduce post-surgical infections and increase wound closure speed.

In conclusion, our studies have shown a major role for HIF-2α in regulating wound healing and highlighted the importance of individually determining the functional role of HIF-1α and HIF-2α in an in vivo physiological setting. We suggest that the epidermal deletion of K14cre-HIF-2α and the K14cre-VHL/HIF-2α is sufficient to increase the anti-microbial activity in the skin and reduce the acute inflammatory response, as shown by lower mRNA expression for MPO and CRAMP. These factors are likely reflected in the unopposed and beneficial effects of the hypoxia-HIF-1α-NOS2-NO pathway in wound repair. Our data predict that the development of a HIF-1α agonist or HIF-2α antagonist would provide a useful adjunct in a surgical setting to help boost the innate immune capacity of the skin, and facilitate wound repair.

Materials & Methods

K14cre-HIF2α and K14cre-VHL/HIF-2α animals

All animals were housed in an approved facility, and experiments conducted in accordance with the National Institute of Health guide for the care and use of laboratory animals. Targeted deletion of HIF-2α or VHL/HIF-2α in keratinocytes was created by crossing mice (C57Bl6/j) homozygous for the floxed allele in HIF-2α or VHL into a background of Cre recombinase expression driven by the K14 promoter, which is specific to cells of the keratinocyte linage(Boutin et al., 2008; Vasioukhin et al., 1999). Deletion efficiency and specificity for the K14cre was determined by comparing tissues from wt and K14cre-HIF1α mice for HIF1α expression. Of the tissues analyzed, only the skin showed a substantial reduction in HIF1α expression (supplemental figure 4) For wound healing assays, the hair on the back of the mice was shaved and depilated 24 h prior to wounding to enable the normal bacterial flora to recover. Mice were anesthetized with 3% isoflurane and a single circular excisional wound of 8 mm diameter generated using a standard sterile biopsy punch that extended full thickness. The animals were caged individually and received buprenorphine at 100 Rg/kg. For wound analysis, mice were euthanized and a standard area 2 mm beyond the original wound margin excised. The wounds were dissected for histology, and analyzed for bacterial flora, and specific mRNA and protein content. The tissues were either fixed in 4% PFA overnight or snap frozen in LN2 and stored at −80°C.

HaCaT scratch assay

HaCaT cells (supplied by CLS Cell Lines Service, Germany), a spontaneously immortalized human keratinocyte line, were propagated in DMEM media supplemented with 10% FCS. Cells were grown to 70% confluence, then transferred to an atmosphere of 1% or 21% O2 for 12 h before scratch injury using a sterile 200 μl pipette tip. Following injury, the media was change to remove cell debris. Digital images were taken from six wells and analyzed for wound closure speed using image J software (NIH).

Morphological and Immunohistochemistry analysis

Skin tissues were excised and fixed in 4% paraformaldehyde, embedded and sectioned in paraffin, and stained with hematoxylin and eosin (Sigma, UK). Digital images were taken on a Leica M165FC microscope using a Leica DFC310FX digital camera (Leica, Milton Keynes, UK). Images were analyzed using Image J software (NIH) and the leading edge equation adopted from Shirakata et al(Shirakata et al., 2005). HIF-1α IHC: Formalin-fixed paraffin-wax embedded skin biopsies were sectioned (4μm) and incubated with monoclonal mouse anti-human HIF1α (1:100) (Novus Biologicals, USA). Antibodies were detected using 3,3′-diaminobenzidine tetrahydrochloride to create a brown reaction product, counterstained with haematoxylin (Dako, UK) and examined by light microscopy.

RNA and DNA analysis

Total RNA was isolated from skin using TRI-reagent (Sigma, UK) followed by RNA clean-up and DNase digest using RNeasy column kits (Qiagen, UK). First-strand synthesis was performed with 1 μg of total RNA using a high-capacity cDNA kit (Applied Biosystems, UK) according to the manufacturers instructions. Relative gene expression was determined by qPCR (ABI Prism 7700 sequence detection system, Applied Biosystems, UK) and amplified in Sybr-green master mix (Applied Biosystems, UK) using relevant primers from Qiagen. Relative gene expression levels were related to β-actin using the 2-CT method(Livak and Schmittgen, 2001). DNA was isolated from tissues using TRI-reagent (Sigma, UK). Taqman qPCR (ABI Step-one plus, Applied Biosystems, UK) for HIF-1α (For 5′-ggtgctggtgtccaaaatgtag Rev 5′-atgggtctagagagatagctccaca, probe 5′-FAMcctgttggttgcgcagcaag) was used to determine deletion efficiency by comparison with VEGF expression (For 5′-tgaccatctgctttcgtgacc, Rev 5′-acttgttgcaggcagcgg, probe 5′-FAMtgctccctgggctcgacagg). 10ng/μl DNA was used per reaction with Taqman universal reaction master mix (Roche, NJ. USA).

Immunoblotting

Tissue samples were lysed in RIPA buffer. A total of 50 μg of whole cell lysate was loaded onto a 4-12% Tris-acetate gel from Invitrogen (NuPAGE®). Immunoblotting analysis was performed using standard methods. The primary antibodies used in this study were: rabbit polyclonals to anti-HIF-1α anti-HIF-2α (1:1000, Novus Biologicals), anti-NOS2, anti-NOS3 and anti-arginase-II (1:200, Santa Cruz Biotechnology). Secondary antibodies used were: goat anti-rabbit IgG-HRP (1:2000, RnD systems).

Statistic analysis

All data represent the mean (± SEM) of (n) separate experiments unless otherwise stated. Differences between groups were assessed using t-test unless otherwise stated. A p value of <0.05 was considered significant.

Supplementary Material

Supplementary Material

Acknowledgements

This work was funded by Cambridge NIHR BRC, Papworth Hospital NHS trust, The Wellcome Trust [WT092738MA], and the National Institutes of Health [5R01AI093451]

Abbreviations

VEGF

Vascular endothelial growth factor

FGF-2

Fibroblasr growth factor-2

PIGF

phosphatidylinositol glycan anchor biosynthesis

ANGPT

angiopoietin 2

myc

myelocytomatosis

MMP

matrix metalloproteinase

NO

nitric oxide

Th1

T-cell helper-1

Th2

T-cell helper-2

CFU

colony forming units

NOS

nitric oxide synthase

MPO

myeloperoxidase

Footnotes

This work was conducted in both: Division of Biological Sciences UCSD, CA, USA and Department of Physiology, Development and Neuroscience. University of Cambridge, Cambridgeshire UK.

Conflicts of Interests: None of the authors report any conflicts of interest.

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