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. 2016 Nov 22;5:37366. doi: 10.1038/srep37366

A mouse model of hereditary hemorrhagic telangiectasia generated by transmammary-delivered immunoblocking of BMP9 and BMP10

Santiago Ruiz 1, Haitian Zhao 1, Pallavi Chandakkar 1, Prodyot K Chatterjee 2, Julien Papoin 3, Lionel Blanc 3,4, Christine N Metz 2,4, Fabien Campagne 5,6, Philippe Marambaud 1,a
PMCID: PMC5118799  PMID: 27874028

Abstract

Hereditary hemorrhagic telangiectasia (HHT) is a potentially life-threatening genetic vascular disorder caused by loss-of-function mutations in the genes encoding activin receptor-like kinase 1 (ALK1), endoglin, Smad4, and bone morphogenetic protein 9 (BMP9). Injections of mouse neonates with BMP9/10 blocking antibodies lead to HHT-like vascular defects in the postnatal retinal angiogenesis model. Mothers and their newborns share the same immunity through the transfer of maternal antibodies during lactation. Here, we investigated whether the transmammary delivery route could improve the ease and consistency of administering anti-BMP9/10 antibodies in the postnatal retinal angiogenesis model. We found that anti-BMP9/10 antibodies, when intraperitoneally injected into lactating dams, are efficiently transferred into the blood circulation of lactationally-exposed neonatal pups. Strikingly, pups receiving anti-BMP9/10 antibodies via lactation displayed consistent and robust vascular pathology in the retina, which included hypervascularization and defects in arteriovenous specification, as well as the presence of multiple and massive arteriovenous malformations. Furthermore, RNA-Seq analyses of neonatal retinas identified an increase in the key pro-angiogenic factor, angiopoietin-2, as the most significant change in gene expression triggered by the transmammary delivery of anti-BMP9/10 antibodies. Transmammary-delivered BMP9/10 immunoblocking in the mouse neonatal retina is therefore a practical, noninvasive, reliable, and robust model of HHT vascular pathology.

Hereditary hemorrhagic telangiectasia (HHT)—also known as Rendu-Osler-Weber syndrome—is an autosomal dominant genetic disease affecting approximately 1 in 5,000–10,000 individuals1,2,3,4. HHT is characterized by the presence of vascular anomalies in multiple tissues and organs in the form of arteriovenous malformations (AVMs) and mucocutaneous telangiectases5,6. These vascular anomalies are structurally compromised and fragile, and hence are susceptible to rupture and hemorrhage. Telangiectases on the skin and in the nasal, oral, and gastrointestinal mucosa, as well as AVMs in the brain, lungs, and liver are typical in the clinical presentation of HHT5,6. Genetic studies have revealed that most HHT patients carry mutations in the genes ENG (encoding endoglin)7 or ACVRL1 (activin receptor-like kinase 1, ALK1)8, which define the two disease subtypes HHT1 and HHT2, respectively9. Mutations in SMAD4 (encoding Smad4)10 and GDF2 (bone morphogenetic protein 9, BMP9)11 were also found to cause rare forms of juvenile polyposis/HHT combined syndrome and HHT-like vascular anomaly syndrome, respectively. Strikingly, BMP9, endoglin, ALK1, and Smad4 all functionally interact in, and are key mediators of, the same BMP receptor signaling pathway. ALK1 is a BMP type I Ser/Thr kinase receptor of the transforming growth factor-β superfamily, which forms functional complexes with a BMP type II receptor (e.g., BMPR2) and the co-receptor endoglin. BMP9 and BMP10 were identified as the specific and physiological ligands for ALK1 in endothelial cells (ECs)12,13,14,15,16,17,18. Upon binding to ALK1-endoglin receptors, BMP9 and BMP10 activate the phosphorylation of receptor-regulated Smads (Smad1, Smad5, and Smad8) to facilitate the formation of Smad1/5/8-Smad4 complexes, which translocate into the nucleus to act as transcription factors in specific gene expression programs19,20.

The exact mechanisms driving HHT pathogenesis remain unknown. However, recent evidence strongly suggests that the disease is caused by abnormal activation of angiogenesis, a process causing excessive EC proliferation and hypervascularization, which ultimately leads to the development of AVMs21. Indeed, ALK1 and endoglin are predominantly expressed in ECs and BMP9/10 signaling is required for proper vascular development and maintenance, as well as for controlling transcriptional responses critically involved in angiogenesis, such as Notch and Wnt signaling pathways22,23,24,25.

Studies in cell lines and animal models have demonstrated that HHT mutations cause haploinsufficiency. Indeed, transfection experiments showed that HHT mutations in either ALK1 or endoglin blocked activation of Smad1/5/8 signaling by BMP926,27,28. The notion that HHT is caused by loss-of-function mutations was strengthened by studies in mouse29 and zebrafish30 models showing that ALK1 or endoglin deficiency, or injection of ALK1 extracellular domain-derived ligand trap (ALK1-Fc), led to vascular hyperproliferation and AVMs. It is important to note that AVMs in some of these models were consistently and robustly observed when ALK1 or endoglin was completely deleted or inhibited, and when precipitating events were in place, such as angiogenesis or inflammation, a process referred to as the double or multiple hit hypothesis29,31. Consistent with these observations, simultaneous neutralization of BMP9 and BMP10 in the postnatal retinal angiogenesis model [by injection of anti-BMP10 antibodies (Abs) into BMP9 knockout (KO) mice, or by co-injection of anti-BMP9 and anti-BMP10 Abs into wild type mice] led to hypervascularization17,18, a vascular defect that was also observed in Acvrl1 or Eng conditional KO models and thus is reminiscent of HHT pathology29.

The postnatal retinal model is commonly used to study physiological or pathological angiogenesis during vascular development. Indeed, the newborn mouse retina is avascular and blood vessels rapidly develop during the first 2 weeks of life through angiogenesis32. This developmental characteristic offers a unique opportunity to study and/or manipulate vascular development, maintenance, and remodeling. In order to improve the BMP9/10 neutralization retinal angiogenesis model, we tested whether the natural transmammary delivery route of administration of BMP9/10 blocking Abs could replace the stressful, cumbersome, and poorly reliable step of individually injecting large numbers of mouse pups.

Neonatal immunity is controlled by passive immunoglobin transfer from the mothers to their newborns during lactation. This mechanism of transmammary delivery of Abs can be very efficient because Abs survive the gastrointestinal tract of the neonates to be absorbed into the blood circulation33. Here we report that BMP9 and BMP10 blocking Abs are efficiently transferred from the mouse dams’ circulation into the blood of their lactationally-exposed neonates to generate a consistent and robust retinal vascular pathology, which was characterized by the presence of key HHT vascular defects. Thus, delivery of BMP9/10 blocking Abs into mouse neonatal pups during lactation produces a practical, noninvasive, reliable, and robust model of HHT vascular pathology.

Results

Transmammary transfer of BMP9 and BMP10 blocking Abs into the circulation of mouse neonates

BMP9 and BMP10 are required, and have overlapping functions, during vascular development in the retina. Consequently, simultaneous injections of BMP9 and BMP10 blocking Abs directly into mouse neonates between postnatal day 1 (P1) and P4 was previously shown to induce strong retinal hypervascularization starting at P517,18. In an effort to improve the ease and consistency of administering Abs to large cohorts of neonates, we investigated whether delivery via the transmammary route was suitable for BMP9/10 neutralization in the retinal angiogenesis model. In this context, we first asked whether BMP9 and BMP10 blocking Abs could transfer from the mouse dams’ blood circulation to the blood of their lactationally-exposed neonates. To this end, lactating dams were injected intraperitoneally once on P3 with monoclonal Abs specific for BMP9 (IgG2b, 15 mg/kg) and BMP10 (IgG2a, 15 mg/kg). As controls, separate sets of dams were injected with the same amount of isotype control IgG2b and IgG2a Abs, or with vehicle only (phosphate-buffered saline, PBS). At P6, neonates were euthanized and the levels of IgG2a and IgG2b Abs in their serum were analyzed by specific anti-IgG2a and anti-IgG2b ELISAs, respectively. We found that neonates fed by dams injected with either anti-BMP9/10 Abs or control IgGs showed a significant and consistent ~3-fold increase in serum IgG2a concentration (which corresponds to an elevation of ~40 μg/mL), when compared to PBS-treated controls (Fig. 1A). An elevation in IgG2b Abs in these neonate serum samples was not detected using the anti-IgG2b ELISA (not shown). Baseline serum concentrations for IgG2b Abs were of ~200 μg/mL, which was approximately 10-fold higher than baseline serum IgG2a levels (~20 μg/mL, Fig. 1A). We believe that these higher levels of baseline IgG2b Abs in neonate serum could have masked any elevation of the concentration of this isotype after the transmammary transfer of IgGs. In this context, we developed an ELISA aimed at specifically detecting anti-BMP9 IgGs in the mouse serum (see Methods). Using this ELISA, we detected the presence of ~30 μg/mL of anti-BMP9 IgGs in the serum of neonates fed by dams injected with the anti-BMP9/10 Abs, whereas, as expected, no anti-BMP9 IgG was measured in serum samples from control IgG-treated or PBS-treated neonates (Fig. 1B). Together, these results show that the transmammary route led to the transfer of both BMP9 and BMP10 blocking Abs to the neonatal blood circulation.

Figure 1. Transmammary transfer of BMP9 and BMP10 blocking Abs into the circulation of mouse neonates.

Figure 1

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(A–D) ELISAs were performed to measure IgG2a (A,C) and anti-BMP9 Ab (B,D) levels in the serum of P6 neonates treated at P3 with vehicle (PBS), isotype control IgGs (IgG2a/2b), or anti-BMP9/10 Abs. Neonates were treated during lactation either from dams injected i.p. with (A,B), or by direct i.p. injections of (C,D), the different Abs or vehicle. Data represent mean ± s.e.m. (n = 5–7 pups per group from 2 dams); ****P < 0.0001, ANOVA.

Next, we compared the serum Ab levels obtained after transmammary delivery to the ones obtained after direct intraperitoneal (i.p.) injections of the pups with the same dose of the two blocking Abs (15 mg/kg). To use comparable protocols, direct injections were also performed once on P3 and serum Ab levels were analyzed on P6. We found that direct Ab injections into the pups led to the accumulation of very similar levels of circulating anti-BMP10 Abs (~30 μg/mL, Fig. 1C) and of about 2-fold more of anti-BMP9 Abs (~50 μg/mL, Fig. 1D), compared to the Ab levels detected after transmammary delivery (Fig. 1A,B). The transmammary delivery route is thus very efficient at administering Abs into the pups’ blood circulation.

Transmammary transfer of BMP9 and BMP10 blocking Abs leads to abnormal hypervascularization of the neonatal retina

The retinal vasculature of P6 neonates was analyzed by histology techniques using isolectin B4 staining. Consistent with the data obtained after direct pup injections of anti-BMP9/10 Abs (refs 17 and 18 and Fig. S1), a robust increase in postnatal retinal vascular density was observed after transmammary transfer of the anti-BMP9/10 Abs, compared to retinas from control IgG-treated or PBS-treated neonates (Fig. 2A–C). Vessel staining revealed the clear presence of a hyperbranched vascular plexus characteristic of a defect in vessel patterning.

Figure 2. Transmammary transfer of BMP9 and BMP10 blocking Abs leads to abnormal hypervascularization in neonatal retinas.

Figure 2

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(A–C”) Representative images of fluorescent isolectin B4-stained retinas either from P6 neonates fed for 3 days by dams injected on P3 with PBS (A), control IgG2a/b Abs (B), or BMP9/10 blocking Abs (C–C”). (C’,C”) are higher magnification images of the relevant boxed areas in C. a, artery; v, vein; scale bars, 500 μm. (D–L) Higher magnification showing retinal vasculature fields between an artery and a vein (Plexus, D–F), or at the front of an artery (G–I) or a vein (J–L) from neonates treated as in (A–C). Scale bars, 100 μm. (M–O) Scatter plots showing the vascular density on retinal ‘petals’ at the plexus (M), artery front (N), or vein front (O). Data represent mean ± s.e.m. (n = 6 pups per group from 2 dams); ****P < 0.0001, ANOVA and Kruskal-Wallis test. Arrows indicate AVMs, defined as direct shunts between an artery and a vein.

We quantified the surface area occupied by the vasculature at the capillary plexus between arteries and veins (Fig. 2D–F), and at the arterial (Fig. 2G–I) and venous (Fig. 2J–L) fronts. We found that, compared to retinas from control IgG-treated or PBS-treated neonates, anti-BMP9/10 Ab transfer significantly increased vascular density (Fig. 2M–O). In addition, the normal alternation of arteries and veins projecting from the optic disk (Fig. 2A,B) was compromised after anti-BMP9/10 Ab transfer (Fig. 2C). Consequently, some vessels could not be anatomically defined as veins or arteries (Fig. 2C), suggesting the presence of a defect in arteriovenous specification upon BMP9/10 immunoblocking.

Transmammary transfer of BMP9 and BMP10 blocking Abs induces AVMs in the neonatal retina

Strikingly, vessel staining also revealed the consistent presence of direct shunts between arteries and veins in neonatal retinas following anti-BMP9/10 Ab transmammary transfer, see arrows in Fig. 2C’, and F. In line with a recent report34, AVMs were also observed after direct pup injections of the two blocking Abs (Fig. S1). To confirm the appearance of these AVMs, injections of latex dye in the blood circulation were used to better visualize pathological arteriovenous shunts in the retina. Because of its size, the latex dye cannot penetrate the capillary beds and thus, in a normal vasculature, is retained in the arterial circulation (see ref. 35 and Fig. 3A for neonatal retinal artery visualization). However, under conditions of anti-BMP9/10 Ab transmammary transfer, the dye invaded the neonatal retinal vein circulation via multiple and, for some of them, very dilated AVMs (arrows, Fig. 3B). In order to quantify these arteriovenous defects, we measured the vascular arborization visualized by the latex dye. To this end, the Sholl’s concentric circle method of dendrite counting in neurons36 was adapted to quantify the number of latex dye-positive vessels. Specifically, a grid of concentric circles equidistantly drawn at 200 μm apart was superimposed at the center of the optic nerve (Fig. 3C) and vascular arborization was determined by counting the number of vascular crosses on the circles. A significant increase in the number of total retinal vascular crosses (Fig. 3D) and on the first 3 concentric circles (Fig. 3E) were found following anti-BMP9/10 Ab transmammary transfer, compared to control IgG-treated or PBS-treated retinas. Thus, anti-BMP9/10 immunoblocking using the transmammary route led to a significant vascular pathology in the retina, which included hypervascularization, defects in arteriovenous specification, and the presence of multiple and massive AVMs.

Figure 3. Transmammary transfer of BMP9 and BMP10 blocking Abs induces AVMs in neonatal retinas.

Figure 3

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(A,B) Representative images of blue latex-perfused retinal vasculature of P6 neonates fed for 3 days by dams injected on P3 with control IgG2a/b Abs (A) or BMP9/10 blocking Abs (B). Arrows in B indicate AVMs. Scale bars, 500 μm. (C) Scheme depicting the method employed for the quantification of the number of latex dye-positive vessels. (D) Histogram showing the total number of vascular crosses. (E) Histogram showing the number of vascular crosses per concentric circle on circles 1 to 3. Data represent mean ± s.e.m. (n = 5–7 pups per group from 2 dams); ****P < 0.0001, ***P < 0.001, **P < 0.01, *P < 0.05; ANOVA and Kruskal-Wallis test (D,E).

Gene expression changes in whole retinas and ECs after ALK1 signaling inhibition

Genome-wide transcriptomic analyses by RNA-Seq were employed to determine whether transmammary-delivered BMP9/10 immunoblocking affects gene expression in the whole retina. Gene expression profiles were analyzed in retinas obtained from neonates following transmammary transfer of anti-BMP9/10 Abs or control IgG2a/2b Abs (n = 6 neonates for each group). This screen identified 128 genes with significant expression changes [False Discovery Rate (FDR) ≤ 1%, absolute log2 fold change ≥0.7, Fig. 4A and Table S1]. Notably, in BMP9/10-immunoblocked retinas, we found a significant increase in the expression of Angpt2 (first hit when sorting by adjusted P-values, log2 fold change = 0.71, adjusted P = 2.69E-08, Limma Voom test, Table 1 and Fig. 4A). Angpt2 codes for angiopoietin-2 (ANG2), a master regulator of sprouting angiogenesis37 that was previously reported to be elevated at the transcriptional level in ALK1 deficient mice38,39. Expression of genes coding for several collagen subunits, including Col4a1 (log2 fold change = 0.70, adjusted P = 1.18E-06) and Col15a1 (log2 fold change = 1.13, adjusted P = 5.05E-05), was also significantly increased in BMP9/10-immunoblocked retinas, compared to control retinas (Table 1 and Fig. 4A). Changes in collagen gene expression is of interest because collagen—and in particular type IV collagen—is a fundamental component of the vascular basement membrane and is key for EC proliferation and survival, and for angiogenesis40. A function enrichment analysis did not reveal any significant network that includes the identified deregulated genes (all categories with FDR > 0.5, GeneMania41).

Figure 4. Gene expression changes in BMP9/10-immunoblocked retinas and ALK1-Fc-treated HUVECs.

Figure 4

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(A) RNA-Seq heat map displaying differently expressed genes in mouse whole retinas following transmammary transfer of anti-BMP9/10 or control IgG2a/2b Abs (n = 6 pups per group from 1 dam). (B) HUVECs were treated or not (Ctrl) with ALK1-Fc (1 μg/mL, 24 h). Cell extracts were then analyzed by WB using Abs directed against the indicated proteins. (C) Densitometric analyses and quantification of phospho-Smad1/5/8, ID1, and ANG2 relative levels in three independent experiments as in (B). (D) ECs isolated from retinas of pups fed for 3 days by dams injected on P3 with control IgG2a/b Abs (Ctrl) or BMP9/10 blocking Abs (anti-BMP9/10) were analyzed for Id1 and Angpt2 mRNA levels by RT-qPCR. The results are expressed as relative levels of the control condition (n = 3 determinations, n = 6 pups per group from 1 dam). Data in (C,D) are mean ± s.e.m.; ***P < 0.001, **P < 0.01, *P < 0.05, unpaired Student’s t-test.

Table 1. Top 25 retinal genes sorted by P-value, following transmammary-delivered immunoblocking of BMP9 and BMP10.

Gene Symbol Ensembl Gene ID Gene Description Log Fold Change Adjusted P-Value
Angpt2 ENSMUSG00000031465 angiopoietin 2 0.71358 2.69E-08
Ighv6-3 ENSMUSG00000076677 immunoglobulin heavy variable 6-3 0.97880 3.77E-08
Sarm1 ENSMUSG00000050132 sterile alpha and HEAT/Armadillo motif containing 1 1.19426 6.39E-08
Pfkp ENSMUSG00000021196 phosphofructokinase, platelet 0.88318 9.18E-08
mt-Tw ENSMUSG00000064346 mitochondrially encoded tRNA tryptophan 0.88100 9.00E-07
mt-Ta ENSMUSG00000064347 mitochondrially encoded tRNA alanine 0.71786 1.02E-06
Col4a1 ENSMUSG00000031502 collagen, type IV, alpha 1 0.70214 1.18E-06
Gga3 ENSMUSG00000020740 golgi associated, gamma adaptin ear containing, ARF binding protein 3 0.98161 6.11E-06
Fitm2 ENSMUSG00000048486 fat storage-inducing transmembrane protein 2 0.97348 7.73E-06
Fam118b ENSMUSG00000050471 family with sequence similarity 118, member B 1.00344 9.88E-06
mt-Tk ENSMUSG00000064355 mitochondrially encoded tRNA lysine 0.91010 1.18E-05
Cd248 ENSMUSG00000056481 CD248 antigen, endosialin 0.87747 2.45E-05
Masp2 ENSMUSG00000028979 mannan-binding lectin serine peptidase 2 −1.03437 2.47E-05
Stab2 ENSMUSG00000035459 stabilin 2 −0.73237 2.76E-05
Fam160a2 ENSMUSG00000044465 family with sequence similarity 160, member A2 0.91040 2.76E-05
Gm13412 ENSMUSG00000085017 predicted gene 13412 1.11272 3.08E-05
Car10 ENSMUSG00000056158 carbonic anhydrase 10 2.50842 3.47E-05
4933431K23Rik ENSMUSG00000086451 RIKEN cDNA 4933431K23 gene 0.93124 3.68E-05
Myo9a ENSMUSG00000039585 myosin IXa 1.07037 4.02E-05
Entpd8 ENSMUSG00000036813 ectonucleoside triphosphate diphosphohydrolase 8 1.15946 4.45E-05
Cbx6 ENSMUSG00000089715 chromobox 6 0.75546 4.45E-05
Gm17828 ENSMUSG00000098893 predicted gene, 17828 −0.87768 4.84E-05
Khsrp ENSMUSG00000007670 KH-type splicing regulatory protein 0.72962 4.84E-05
Col15a1 ENSMUSG00000028339 collagen, type XV, alpha 1 1.13494 5.05E-05
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The first 25 genes with adjusted P-value (false discovery rate) less or equal to 1%, and abs(logFC) ≥ 0.7, sorted by increasing adjusted P-value, are shown. Gene expression changes are expressed in log2 fold change and compare anti-BMP9/10 Ab-treated versus control IgG2a/2b-treated retinas. Positive logFC values denote genes over-expressed in anti-BMP9/10 Ab-treated retinas. A log2 fold change value of 1 corresponds to a doubling of expression in treated retinas (log2(2) = 1).

To confirm the effect of ALK1 inhibition on global gene expression and to determine which deregulations originate from ECs, we also performed RNA-Seq on human umbilical vein endothelial cells (HUVECs) treated or not with the ligand trap ALK1-Fc. Comparison of the gene expression profiles obtained from BMP9/10-immunoblocked neonatal retinas and ALK1-Fc-treated HUVECs validated the increase of ANG2 expression upon ALK1 signaling inhibition. Indeed, ALK1-Fc treatment significantly increased ANGPT2 RNA levels in HUVECs (log2 fold change = 0.32, adjusted P = 2.99E-06). These results are important because they confirmed that ALK1 signaling is an endogenous repressor of ANG2 expression in ECs. In order to confirm at the protein level the effect of ALK1 signaling inhibition on ANG2 expression, we analyzed ANG2 levels by western blot (WB) in ALK1-Fc-treated HUVECs. As expected, we found that ALK1-Fc treatment strongly suppressed ALK1 signaling, which was manifested by a decrease in the activating phosphorylation of Smad1/5/8 and in the protein levels of inhibitor of differentiation 1 (ID1), two downstream targets and effectors of ALK1 activation (Fig. 4B,C). Importantly and in line with the RNA-Seq data, we found that ALK1-Fc treatment of HUVECs significantly increased ANG2 protein levels (Fig. 4B,C). To go further, we performed RT-qPCR analyses on ECs isolated from P6 mouse pup retinas using anti-CD31 microbeads. These analyses confirmed that transmammary-delivered BMP9/10 immunoblocking significantly reduced Id1 expression and increased Angpt2 expression (Fig. 4D). Thus, transmammary-delivered BMP9/10 immunoblocking inhibited ALK1 signaling in vivo in retinal ECs and derepressed ANG2 expression.

Together these results show that, at the autonomous level in ECs, ALK1 signaling negatively controlled the expression of the key pro-angiogenic mediator ANG2. Consequently, inhibition of ALK1 signaling in the presented model triggered a pathological pro-angiogenic response that led to hypervascularization and AVMs.

Discussion

The first HHT mouse models developed were constitutive Acvrl1 and Eng KO mice. Based on the loss-of-function mutation paradigm in HHT, heterozygous KO mice for Acvrl1 or Eng were expected to exemplify the most representative models for this disease. However, Acvrl1+/− and Eng+/− mice only displayed mild phenotypes with variable HHT-like vascular defects from one genetic background to another29. More recently, powerful inducible conditional KO mice for Acvrl1 or Eng were generated35,42,43. Complete knockdown of either Acvrl1 or Eng in these models led to more robust and reliable phenotypes, which included the appearance of AVMs29. It is important to note that in these models, complete Acvrl1- or Eng-deficiency per se was found not to be sufficient for generating the observed vascular defects and that additional triggers in the form of inflammatory and/or angiogenic stimuli were required at the sites where AVMs developed29,31,35. Together with the observation that homozygous Acvrl1 or Eng KO mice die at an early embryonic stage most likely from angiogenesis defects, these data highlight the existence of a clear interplay between angiogenesis and ALK1-endoglin signaling. Evidence is indeed strong to indicate that ALK1-endoglin signaling is necessary for the proper expression of angiogenesis in certain tissues, and that angiogenic stimuli, in return, can provide a trigger for the development of HHT phenotypes in models defective for ALK1-endoglin signaling. For instance, treatments with the master initiator of sprouting angiogenesis VEGF44 facilitated the development of vascular dysplasia in Acvrl1 and Eng KO mice45,46, and VEGF neutralization using bevacizumab was found to be effective at interfering with AVM development and progression in the wound-induced AVM mouse model47. These observations are in line with several early-phase clinical trials supporting that bevacizumab treatments—using topical, submucosal, or i.v. infusion routes—were effective at reducing epistaxis in HHT patients48,49,50, but see also refs 51 and 52.

In this context, the postnatal retinal angiogenesis model is very attractive for studying HHT vascular pathology. Indeed, physiological angiogenesis, which is required for postnatal vascular development, will provide the required additional trigger for vascular pathology development in mice deficient for ALK1 or endoglin expression42,53 or in mice treated with BMP9/10 blocking Abs17,18. An important advantage of this model is the rapid pathology occurrence during the first week of postnatal vascular development. The use of BMP9/10 blocking Abs provides an additional advantage—over Acvrl1 or Eng KO mice—which is that Abs can be injected into any mouse strain, avoiding the phenotypic variability sometimes observed between mutant mice of different and complex genetic backgrounds29.

For these reasons and in the current study, we sought to improve the practicality and reliability of the neonatal retinal angiogenesis model of BMP9/10 immunoblocking. Based on strong supporting literature showing that neonatal immunity is controlled by passive immunoglobin transfer from mothers to their newborns during lactation, we asked whether the transmammary route could be used to deliver BMP9/10 blocking Abs into mouse neonates. We found for the first time that these Abs were very efficiently transferred from the dam’s circulation to the neonates’ blood during lactation. In addition, this transfer triggered the development of a robust and consistent retinal vascular pathology, which included hypervascularization, partial loss of arteriovenous specification, and most importantly, AVMs.

In this study, we compared the vascular pathology generated by the blocking Abs using the transmammary route and the direct injections of the pups. We found that injection of the same amount of anti-BMP9 and anti-BMP10 blocking Abs (15 mg/kg), and using the same procedure timing (one injection at P3 and retinal analysis at P6), showed that both approaches led to hypervascularization, but also and as recently reported34, to AVM development. It should be noted, however, that the original studies describing the direct injection method17,18 did not identify AVMs in their models. The exact reason for this difference in AVM development using the direct injection route remains unexplained, but we note that the anti-BMP9/10 Ab injection timing was different between the original studies17,18 (Ab injections starting at P1) and the studies showing AVM development (Ab injections at P3, this study and ref. 34). Ab injections at an earlier time point during retinal vascular development could explain the more aggressive inhibitory effect on vascular expansion observed in the original reports17,18,34. It is thus possible that AVMs require a certain level of vascular development and expansion, which is only reached when anti-BMP9/10 blocking Abs are administered after a certain level of development; i.e., at P3. This level of vascular development and expansion would in turn allow the establishment of a normal blood flow, which was shown to interact with ALK1 signaling to facilitate AVM development34,54,55. Future studies comparing different injection timings with anti-BMP9/10 blocking Abs will be required to test this possibility.

Using whole transcriptome analyses in the neonatal retina, we found in this study a significant elevation of Angpt2 expression following anti-BMP9/10 Ab transmammary delivery. Whole transcriptome analyses of ALK1-Fc-treated HUVECs and RT-qPCR analyses in ECs isolated from BMP9/10-immunoblocked pup retinas confirmed the effect of ALK1 signaling inhibition on Angpt2 expression and also showed that ALK1 inhibition increased Angpt2 expression in an EC-autonomous manner. WB analyses of ALK1-Fc-treated HUVECs confirmed that inhibiting ALK1 signaling significantly increased ANG2 protein levels. Together, these data demonstrate that ALK1 signaling is a physiological repressor of ANG2 expression in ECs. This observation is consistent with previous data showing that ANG2 expression is increased in ALK1−/− embryos38 and adult ALK1+/− lung tissue39, as well as in conditional ALK1 KO mouse models of central nervous system AVMs56. Increases in ANG2 expression were also reported in the plasma and plexiform lesions of patients affected by pulmonary arterial hypertension (PAH), a condition that can be caused by mutations in ALK1 or BMPR257. These data, however, contrast with the observation that ANG2 levels might be reduced in the plasma of a small cohort of HHT2 patients, but not in HHT1 patients58. In this context, our data strengthen the concept that ANG2 might be a crucial trigger of the vascular pathology caused by ALK1 signaling loss-of-function, and beyond that, for HHT pathogenesis. ANG2 is a circulating ligand that, in conjunction with VEGF signaling, has critical pro-angiogenic properties during the induction of vascular sprouting59. Knowing that ANG2 is currently being investigated as a potential target for anti-angiogenic tumor therapy60, it is tempting to speculate that anti-ANG2 approaches might also have therapeutic value in HHT.

A gene that also showed deregulated expression, albeit with less consistency inside the groups, was Ccm2 (log2 fold change = 2.44, adjusted P = 1.72E-04, see Fig. 4A and Table S1). Ccm2 is of interest because it codes for malcavernin, a protein that mediates interactions between blood vessel cells. Mutations have been identified in the CCM2 human ortholog gene in patients with familial cerebral cavernous malformation (CCM)61. CCM leads to vascular malformations mostly in the brain, but also in other tissues, and its phenotype is closely related to, albeit different from, the AVMs observed in HHT patients: CCMs are low-flow lesions, while HHT AVMs are high-flow lesions62. Furthermore, while loss-of-function mutations in CCM2 are associated with CCM in humans, in our model of BMP9/10-immunoblocking, we observed an increase of Ccm2 expression, suggesting the possible existence of a compensatory mechanism that mitigates the vascular changes induced by ALK1 signaling inactivation. Further studies will be required to address this possible mechanism and determine whether CCM2 deregulations might also be associated with AVM development in HHT.

In conclusion, we propose that transmammary-delivered immunoblocking of BMP9 and BMP10 in the mouse neonatal retina is a practical, noninvasive, reliable, and robust model to study HHT pathogenesis. Furthermore, this study provides proof-of-concept data that the described model is suitable for mechanistic and ultimately, pre-clinical therapeutic investigations for HHT. From a more general standpoint and to the best of our knowledge, the paradigm described here represents the first example of generation of an infection-unrelated disease model utilizing dam/neonate-shared immunity.

Materials and Methods

Mice

All animal procedures were performed in accordance with protocols approved by the Feinstein Institute for Medical Research Institutional Animal Care and Use Committee. Timed-pregnant C57BL/6J mice (3–4 month old) were used in this study (The Jackson Laboratory).

Ab injections and transmammary transfer of Abs via lactation

Lactating dams were injected i.p. once on P3 with PBS, mouse monoclonal isotype control Abs (15 mg/kg, IgG2b, MAB004; 15 mg/kg, IgG2a, MAB003; R&D Systems), or mouse monoclonal anti-BMP9 and anti-BMP10 Abs (15 mg/kg, IgG2b, MAB3209; 15 mg/kg, IgG2a, MAB2926; R&D Systems, respectively). As controls, groups of neonates were directly injected i.p. on P3 with PBS or the same mouse monoclonal isotype control or anti-BMP9 and anti-BMP10 Abs (15 mg/kg). Neonates were euthanized by CO2 asphyxiation on P6 and non-heparinized blood was collected. Neonates were enucleated and eyes fixed in 4% paraformaldehyde for 20 min on ice and retinas were isolated.

Measurements of Ab levels by ELISA in neonatal mouse serum

ELISAs were used to measure IgG2a, IgG2b, and anti-BMP9 Ab levels in mouse serum. IgG2a and IgG2b ELISAs were performed as per the manufacturer’s instructions (eBioscience). For the anti-BMP9 Ab ELISA, 96-well ELISA plates (Maxisorp, Nunc) were coated with 100 μL of 1 μg/mL recombinant BMP9 (R&D Systems) in coating buffer (15 mM K2HPO4, 25 mM KH2PO4, 0.1 M NaCl2, 0.1 mM EDTA, 7.5 mM NaN3) and incubated overnight at 4 °C. Plates were then washed 3 times with 0.05% Tween PBS (PBST) and blocked for 1 h at room temperature (RT) with 1% BSA in PBS. After washing 3 times with PBST, serial dilutions of individual mouse serum samples and reference mouse anti-BMP9 Ab (MAB3209, R&D Systems) (diluted in 1% BSA PBS) were prepared and 100 μL/well were incubated for 2 h at RT. After 3 more washes, 100 μL/well horseradish peroxidase (HRP)-conjugated goat anti-mouse immunoglobins (Igs) secondary Ab (Southern Biotech, diluted 1:500 in 1% BSA PBS) was incubated for 1 h at RT. TMB substrate was added after 5 washes and the reaction was allowed to develop for 30 min at RT. The optical density was measured at 450 nm using a TECAN GENios Pro plate reader.

Retinal whole mount immunohistochemistry (IHC)

IHC was performed using the previously described protocol63 with the following modifications. After fixation using 4% paraformaldehyde, retinas were dissected, cut four times to flatten them into petal flower shapes, and fixed with methanol for 20 min on ice. After removing methanol, retinas were washed in PBS for 5 min on a shaker at RT, and blocked in blocking solution (0.3% Triton, 0.2% BSA in PBS) for 1 h on a shaker at RT. Retinas were then incubated in isolectin GS-IB4 Alexa Fluor 488 (I21411, Molecular Probes) diluted 1:100 in blocking solution on a shaker overnight at 4 °C. Retinas were then washed four times in 0.3% Triton in PBS for 10 min on a shaker, followed by two washes in PBS for 5 min on a shaker before mounting with Vecta Shield (H-1000, Vector Laboratories).

Blue latex perfusion assay

The blue latex perfusion assay was performed using a previously described protocol35, with the following modifications. Briefly, after euthanasia, neonate thoraxes were opened using Dumont #5 forceps and an extra fine Bonn scissor (Fine Science Tools Inc.). The right atriums were cut using a Vannas spring scissor (Fine Science Tools Inc.), and the left ventricles were injected manually with 1 mL Blue latex (BR 80B, Connecticut Valley Biological Supply) using an insulin syringe U-100 (329652, BD Biosciences). After perfusion, eyes were enucleated and fixed, and retinas were dissected for microscopic observation as described above.

Image acquisition and analysis

Images for the analysis of the vascular network density were acquired using a laser confocal microscopy Olympus FV300, while images for the analysis of the number of crosses of arteries and veins were acquired using a Nikon Eclipse T2000-S microscope. Quantifications were performed using ImageJ. Using a 20x lens, images (2–5 fields per retina) were acquired in three different locations of the vasculature: The plexus (between an artery and a vein) and the front of the extending arterial and venous vasculature. Quantification was done using the measure particles tool, working with 8-bit images, adjusting the threshold, and measuring the area occupy by the vasculature in a region of interest of 200 × 200 μm2 in these three locations. For the analysis of the number of artery and vein crosses, whole retinas were imaged with a 4x lens. Quantification was performed using the counter tool and plug-in concentric circles, counting each crossing artery and vein on 5 concentric circles equidistantly drawn (200 μm apart) from the optic nerve to the periphery of the extending vasculature of the retina.

Statistical analysis

ANOVA was used to assess statistical significance within multiple comparisons analyses. When data had non-normal distribution, Kruskal-Wallis test was performed instead. Tukey’s or Dunn’s multiple comparisons test were performed as post hoc tests. In all cases GraphPad Prism version 6.0 was used.

Retinal RNA extraction and sequencing

After euthanasia, neonate eyes were enucleated and retinas dissected in PBS. Retinas were rapidly dried with absorbent paper, snap-frozen in liquid nitrogen and stored at −80 °C. RNA was then extracted from retinas using the RNeasy Micro Kit (Qiagen) according to the manufacturer’s instructions. Total RNA quality was verified using Thermo Scientific NanoDrop and Agilent Bioanalyzer. RNA was processed for RNA-Seq at the Genomics Resources Core Facility, Weill Cornell Medical College, New York, NY. Briefly, cDNA conversion and library preparation were performed using the TrueSeq v2 Illumina library preparation kit, following the manufacturers’ recommended protocol. Samples were multiplexed 6 per lane and sequenced on an Illumina HiSeq 4000 instrument.

RNA-Seq data analysis

Reads were uploaded to the GobyWeb system64 and aligned to the 1000 genome human reference sequence65 with the STAR aligner66. Ensembl annotations for transcripts were obtained from Biomart and Ensembl automatically using GobyWeb. Annotations were used to determine read counts using the Goby alignment-to-annotation-counts mode67, integrated in GobyWeb in the differential expression analysis with EdgeR plugin. Counts were downloaded from GobyWeb as a tab delimited file and analyzed with MetaR68. Statistical analyses were conducted with Limma Voom69, as integrated in MetaR 1.7.2, using the rocker-metar docker image version 1.6.0.1. P-values were adjusted for multiple testing using the False Discovery Rate (FDR) method70. Heat maps were constructed with MetaR, using the pheatmap R package. Gene annotations were determined with Ensembl/Biomart, using the biomart micro-language in MetaR68. MetaR analysis scripts are presented in Supplementary Material (Figs S2–S5).

Retinal EC isolation and RT-qPCR

ECs were isolated from neonatal retinal tissue using anti-CD31 microbeads, as per the manufacturer’s instructions (Miltenyi Biotec GmbH). One-step RT-qPCR was performed on pellets of 40–60,000 cells per sample using Cells-to-CtTM 1-Step TaqMan® Kit following the manufacturer’s protocol (Ambion, Thermo Fisher Scientific Inc.). PCR was performed using TaqMan assays on ABI 7900 HT (Applied Biosystems, Life Technologies). Angpt2 and Id1 expression levels were normalized to the reference gene Polr2a. Relative changes in gene expression were determined by the ΔΔCt method71 and using isotype control values normalized to 1.0.

HUVEC cultures, treatments, RNA extraction, and western blot (WB) analyses

HUVECs were isolated from anonymous umbilical veins, as described before72. HUVECs were subcultured using a trypsin/EDTA-reagent pack (Lonza) and maintained in 5% fetal bovine serum (FBS)-containing EC growth medium (Sciencell). Cells were treated or not for 24 h with 1 μg/mL ALK1-Fc (R&D Systems) in complete EC growth medium containing 5% FBS. Cells were then rinsed with PBS and processed for RNA extraction and RNA-Seq as described above. For WB analyses, cells were processed as before73 with the following modifications. Cells were solubilized in RIPA buffer (EMD Millipore) supplemented with 1× Complete protease inhibitor mixture (Roche Applied Science). 5–20 μg of proteins (depending on the primary Ab used) were separated by SDS-PAGE and transferred onto nitrocellulose membranes. Membranes were then probed with Abs directed against phospho-Smad1/5/8 (Cell Signaling Technology), total Smad5 (Cell Signaling Technology), ID1 (BioCheck), ANG2 (Santa Cruz Biotechnology), and actin (BD Transduction Laboratories). A standard ECL detection procedure was then used.

Additional Information

Accession Codes: RNA-Seq reads have been deposited to the Sequence Read Archive under accession code SRP071883

How to cite this article: Ruiz, S. et al. A mouse model of hereditary hemorrhagic telangiectasia generated by transmammary-delivered immunoblocking of BMP9 and BMP10. Sci. Rep. 6, 37366; doi: 10.1038/srep37366 (2016).

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Supplementary Material

Supplementary Information
srep37366-s1.xls (87KB, xls)
Supplementary Information
srep37366-s2.pdf (4.7MB, pdf)

Acknowledgments

This work was supported by a Feinstein Institute for Medical Research fund (to P.M.).

Footnotes

Author Contributions S.R., H.Z., P.C., P.K.C. and J.P. performed the experiments and analyzed the data. F.C. performed the bioinformatic analyses of the RNA-Seq data. P.M. conceived the project and elaborated the experimental strategy with S.R., L.B., C.N.M. and F.C.; P.M., S.R., F.C., L.B., and C.N.M. wrote the manuscript.

References

  1. Guttmacher A. E., Marchuk D. A. & White R. I. Hereditary hemorrhagic telangiectasia. N Engl J Med 333, 918–924, doi: 10.1056/NEJM199510053331407 (1995). [DOI] [PubMed] [Google Scholar]
  2. Richards-Yutz J., Grant K., Chao E. C., Walther S. E. & Ganguly A. Update on molecular diagnosis of hereditary hemorrhagic telangiectasia. Hum Genet 128, 61–77, doi: 10.1007/s00439-010-0825-4 (2010). [DOI] [PubMed] [Google Scholar]
  3. Marchuk D. A., Guttmacher A. E., Penner J. A. & Ganguly P. Report on the workshop on Hereditary Hemorrhagic Telangiectasia, July 10–11, 1997. Am J Med Genet 76, 269–273 (1998). [PubMed] [Google Scholar]
  4. Arthur H. et al. Executive summary of the 11th HHT international scientific conference. Angiogenesis 18, 511–524, doi: 10.1007/s10456-015-9482-5 (2015). [DOI] [PubMed] [Google Scholar]
  5. Dupuis-Girod S., Bailly S. & Plauchu H. Hereditary hemorrhagic telangiectasia: from molecular biology to patient care. J Thromb Haemost 8, 1447–1456, doi: 10.1111/j.1538-7836.2010.03860.x (2010). [DOI] [PubMed] [Google Scholar]
  6. Shovlin C. L. Hereditary haemorrhagic telangiectasia: pathophysiology, diagnosis and treatment. Blood Rev 24, 203–219, doi: 10.1016/j.blre.2010.07.001 (2010). [DOI] [PubMed] [Google Scholar]
  7. McAllister K. A. et al. Endoglin, a TGF-beta binding protein of endothelial cells, is the gene for hereditary haemorrhagic telangiectasia type 1. Nat Genet 8, 345–351, doi: 10.1038/ng1294-345 (1994). [DOI] [PubMed] [Google Scholar]
  8. Johnson D. W. et al. Mutations in the activin receptor-like kinase 1 gene in hereditary haemorrhagic telangiectasia type 2. Nat Genet 13, 189–195, doi: 10.1038/ng0696-189 (1996). [DOI] [PubMed] [Google Scholar]
  9. McDonald J. et al. Hereditary hemorrhagic telangiectasia: genetics and molecular diagnostics in a new era. Front Genet 6, 1, doi: 10.3389/fgene.2015.00001 (2015). [DOI] [PMC free article] [PubMed] [Google Scholar]
  10. Gallione C. J. et al. A combined syndrome of juvenile polyposis and hereditary haemorrhagic telangiectasia associated with mutations in MADH4 (SMAD4). Lancet 363, 852–859, doi: 10.1016/S0140-6736(04)15732-2 (2004). [DOI] [PubMed] [Google Scholar]
  11. Wooderchak-Donahue W. L. et al. BMP9 mutations cause a vascular-anomaly syndrome with phenotypic overlap with hereditary hemorrhagic telangiectasia. Am J Hum Genet 93, 530–537, doi: 10.1016/j.ajhg.2013.07.004 (2013). [DOI] [PMC free article] [PubMed] [Google Scholar]
  12. David L., Mallet C., Mazerbourg S., Feige J. J. & Bailly S. Identification of BMP9 and BMP10 as functional activators of the orphan activin receptor-like kinase 1 (ALK1) in endothelial cells. Blood 109, 1953–1961, doi: 10.1182/blood-2006-07-034124 (2007). [DOI] [PubMed] [Google Scholar]
  13. Scharpfenecker M. et al. BMP-9 signals via ALK1 and inhibits bFGF-induced endothelial cell proliferation and VEGF-stimulated angiogenesis. J Cell Sci 120, 964–972, doi: 10.1242/jcs.002949 (2007). [DOI] [PubMed] [Google Scholar]
  14. David L. et al. Bone morphogenetic protein-9 is a circulating vascular quiescence factor. Circ Res 102, 914–922, doi: 10.1161/CIRCRESAHA.107.165530 (2008). [DOI] [PMC free article] [PubMed] [Google Scholar]
  15. Brown M. A. et al. Crystal structure of BMP-9 and functional interactions with pro-region and receptors. J Biol Chem 280, 25111–25118, doi: 10.1074/jbc.M503328200 (2005). [DOI] [PubMed] [Google Scholar]
  16. Li W., Salmon R. M., Jiang H. & Morrell N. W. Regulation of the ALK1 ligands, BMP9 and BMP10. Biochem Soc Trans 44, 1135–1141, doi: 10.1042/BST20160083 (2016). [DOI] [PubMed] [Google Scholar]
  17. Chen H. et al. Context-dependent signaling defines roles of BMP9 and BMP10 in embryonic and postnatal development. Proc Natl Acad Sci USA 110, 11887–11892, doi: 10.1073/pnas.1306074110 (2013). [DOI] [PMC free article] [PubMed] [Google Scholar]
  18. Ricard N. et al. BMP9 and BMP10 are critical for postnatal retinal vascular remodeling. Blood 119, 6162–6171, doi: 10.1182/blood-2012-01-407593 (2012). [DOI] [PMC free article] [PubMed] [Google Scholar]
  19. Massagué J. TGFβ signalling in context. Nat Rev Mol Cell Biol 13, 616–630, doi: 10.1038/nrm3434 (2012). [DOI] [PMC free article] [PubMed] [Google Scholar]
  20. Cai J., Pardali E., Sánchez-Duffhues G. & ten Dijke P. BMP signaling in vascular diseases. FEBS Lett 586, 1993–2002, doi: 10.1016/j.febslet.2012.04.030 (2012). [DOI] [PubMed] [Google Scholar]
  21. Ardelean D. S. & Letarte M. Anti-angiogenic therapeutic strategies in hereditary hemorrhagic telangiectasia. Front Genet 6, 35, doi: 10.3389/fgene.2015.00035 (2015). [DOI] [PMC free article] [PubMed] [Google Scholar]
  22. García de Vinuesa A., Abdelilah-Seyfried S., Knaus P., Zwijsen A. & Bailly S. BMP signaling in vascular biology and dysfunction. Cytokine Growth Factor Rev 27, 65–79, doi: 10.1016/j.cytogfr.2015.12.005 (2016). [DOI] [PubMed] [Google Scholar]
  23. Larrivée B. et al. ALK1 signaling inhibits angiogenesis by cooperating with the Notch pathway. Dev Cell 22, 489–500, doi: 10.1016/j.devcel.2012.02.005 (2012). [DOI] [PMC free article] [PubMed] [Google Scholar]
  24. Choi E. J. et al. Enhanced responses to angiogenic cues underlie the pathogenesis of hereditary hemorrhagic telangiectasia 2. PLoS One 8, e63138, doi: 10.1371/journal.pone.0063138 (2013). [DOI] [PMC free article] [PubMed] [Google Scholar]
  25. Aspalter I. M. et al. Alk1 and Alk5 inhibition by Nrp1 controls vascular sprouting downstream of Notch. Nat Commun 6, 7264, doi: 10.1038/ncomms8264 (2015). [DOI] [PMC free article] [PubMed] [Google Scholar]
  26. Alaa El Din F. et al. Functional and splicing defect analysis of 23 ACVRL1 mutations in a cohort of patients affected by Hereditary Hemorrhagic Telangiectasia. PLoS One 10, e0132111, doi: 10.1371/journal.pone.0132111 (2015). [DOI] [PMC free article] [PubMed] [Google Scholar]
  27. Ricard N. et al. Functional analysis of the BMP9 response of ALK1 mutants from HHT2 patients: a diagnostic tool for novel ACVRL1 mutations. Blood 116, 1604–1612, doi: 10.1182/blood-2010-03-276881 (2010). [DOI] [PubMed] [Google Scholar]
  28. Mallet C. et al. Functional analysis of endoglin mutations from hereditary hemorrhagic telangiectasia type 1 patients reveals different mechanisms for endoglin loss of function. Hum Mol Genet 24, 1142–1154, doi: 10.1093/hmg/ddu531 (2015). [DOI] [PubMed] [Google Scholar]
  29. Tual-Chalot S., Oh S. P. & Arthur H. M. Mouse models of hereditary hemorrhagic telangiectasia: recent advances and future challenges. Front Genet 6, 25, doi: 10.3389/fgene.2015.00025 (2015). [DOI] [PMC free article] [PubMed] [Google Scholar]
  30. Rochon E. R., Menon P. G. & Roman B. L. Alk1 controls arterial endothelial cell migration in lumenized vessels. Development 143, 2593–2602, doi: 10.1242/dev.135392 (2016). [DOI] [PMC free article] [PubMed] [Google Scholar]
  31. López-Novoa J. M. & Bernabeu C. The physiological role of endoglin in the cardiovascular system. Am J Physiol Heart Circ Physiol 299, H959–H974, doi: 10.1152/ajpheart.01251.2009 (2010). [DOI] [PubMed] [Google Scholar]
  32. Stahl A. et al. The mouse retina as an angiogenesis model. Invest Ophthalmol Vis Sci 51, 2813–2826, doi: 10.1167/iovs.10-5176 (2010). [DOI] [PMC free article] [PubMed] [Google Scholar]
  33. Hurley W. L. & Theil P. K. Perspectives on immunoglobulins in colostrum and milk. Nutrients 3, 442–474, doi: 10.3390/nu3040442 (2011). [DOI] [PMC free article] [PubMed] [Google Scholar]
  34. Baeyens N. et al. Defective fluid shear stress mechanotransduction mediates hereditary hemorrhagic telangiectasia. J Cell Biol, doi: 10.1083/jcb.201603106 (2016). [DOI] [PMC free article] [PubMed] [Google Scholar]
  35. Park S. O. et al. Real-time imaging of de novo arteriovenous malformation in a mouse model of hereditary hemorrhagic telangiectasia. J Clin Invest 119, 3487–3496, doi: 10.1172/JCI39482 (2009). [DOI] [PMC free article] [PubMed] [Google Scholar]
  36. Sholl D. A. Dendritic organization in the neurons of the visual and motor cortices of the cat. J Anat 87, 387–406 (1953). [PMC free article] [PubMed] [Google Scholar]
  37. Eklund L. & Saharinen P. Angiopoietin signaling in the vasculature. Exp Cell Res 319, 1271–1280, doi: 10.1016/j.yexcr.2013.03.011 (2013). [DOI] [PubMed] [Google Scholar]
  38. Oh S. P. et al. Activin receptor-like kinase 1 modulates transforming growth factor-beta 1 signaling in the regulation of angiogenesis. Proc Natl Acad Sci USA 97, 2626–2631 (2000). [DOI] [PMC free article] [PubMed] [Google Scholar]
  39. Ardelean D. S. et al. Endoglin and activin receptor-like kinase 1 heterozygous mice have a distinct pulmonary and hepatic angiogenic profile and response to anti-VEGF treatment. Angiogenesis 17, 129–146, doi: 10.1007/s10456-013-9383-4 (2014). [DOI] [PubMed] [Google Scholar]
  40. Mundel T. M. & Kalluri R. Type IV collagen-derived angiogenesis inhibitors. Microvasc Res 74, 85–89, doi: 10.1016/j.mvr.2007.05.005 (2007). [DOI] [PMC free article] [PubMed] [Google Scholar]
  41. Warde-Farley D. et al. The GeneMANIA prediction server: biological network integration for gene prioritization and predicting gene function. Nucleic Acids Res 38, W214–W220, doi: 10.1093/nar/gkq537 (2010). [DOI] [PMC free article] [PubMed] [Google Scholar]
  42. Tual-Chalot S. et al. Endothelial depletion of Acvrl1 in mice leads to arteriovenous malformations associated with reduced endoglin expression. PLoS One 9, e98646, doi: 10.1371/journal.pone.0098646 (2014). [DOI] [PMC free article] [PubMed] [Google Scholar]
  43. Garrido-Martin E. M. et al. Common and distinctive pathogenetic features of arteriovenous malformations in hereditary hemorrhagic telangiectasia 1 and hereditary hemorrhagic telangiectasia 2 animal models–brief report. Arterioscler Thromb Vasc Biol 34, 2232–2236, doi: 10.1161/ATVBAHA.114.303984 (2014). [DOI] [PubMed] [Google Scholar]
  44. Carmeliet P. & Jain R. K. Molecular mechanisms and clinical applications of angiogenesis. Nature 473, 298–307, doi: 10.1038/nature10144 (2011). [DOI] [PMC free article] [PubMed] [Google Scholar]
  45. Xu B. et al. Vascular endothelial growth factor induces abnormal microvasculature in the endoglin heterozygous mouse brain. J Cereb Blood Flow Metab 24, 237–244, doi: 10.1097/01.WCB.0000107730.66603.51 (2004). [DOI] [PubMed] [Google Scholar]
  46. Hao Q. et al. VEGF Induces More Severe Cerebrovascular Dysplasia in Endoglin than in Alk1 Mice. Transl Stroke Res 1, 197–201, doi: 10.1007/s12975-010-0020-x (2010). [DOI] [PMC free article] [PubMed] [Google Scholar]
  47. Han C. et al. VEGF neutralization can prevent and normalize arteriovenous malformations in an animal model for hereditary hemorrhagic telangiectasia 2. Angiogenesis 17, 823–830, doi: 10.1007/s10456-014-9436-3 (2014). [DOI] [PMC free article] [PubMed] [Google Scholar]
  48. Thompson A. B. et al. Very low dose bevacizumab for the treatment of epistaxis in patients with hereditary hemorrhagic telangiectasia. Allergy Rhinol (Providence) 5, 91–95, doi: 10.2500/ar.2014.5.0091 (2014). [DOI] [PMC free article] [PubMed] [Google Scholar]
  49. Karnezis T. T. & Davidson T. M. Treatment of hereditary hemorrhagic telangiectasia with submucosal and topical bevacizumab therapy. Laryngoscope 122, 495–497, doi: 10.1002/lary.22501 (2012). [DOI] [PubMed] [Google Scholar]
  50. Dupuis-Girod S. et al. Bevacizumab in patients with hereditary hemorrhagic telangiectasia and severe hepatic vascular malformations and high cardiac output. JAMA 307, 948–955, doi: 10.1001/jama.2012.250 (2012). [DOI] [PubMed] [Google Scholar]
  51. Dupuis-Girod S. et al. Effect of Bevacizumab Nasal Spray on Epistaxis Duration in Hereditary Hemorrhagic Telangectasia: A Randomized Clinical Trial. JAMA 316, 934–942, doi: 10.1001/jama.2016.11387 (2016). [DOI] [PubMed] [Google Scholar]
  52. Whitehead K. J. et al. Effect of Topical Intranasal Therapy on Epistaxis Frequency in Patients With Hereditary Hemorrhagic Telangiectasia: A Randomized Clinical Trial. JAMA 316, 943–951, doi: 10.1001/jama.2016.11724 (2016). [DOI] [PubMed] [Google Scholar]
  53. Mahmoud M. et al. Pathogenesis of arteriovenous malformations in the absence of endoglin. Circ Res 106, 1425–1433, doi: 10.1161/CIRCRESAHA.109.211037 (2010). [DOI] [PubMed] [Google Scholar]
  54. Corti P. et al. Interaction between alk1 and blood flow in the development of arteriovenous malformations. Development 138, 1573–1582, doi: 10.1242/dev.060467 (2011). [DOI] [PMC free article] [PubMed] [Google Scholar]
  55. Laux D. W. et al. Circulating Bmp10 acts through endothelial Alk1 to mediate flow-dependent arterial quiescence. Development 140, 3403–3412, doi: 10.1242/dev.095307 (2013). [DOI] [PMC free article] [PubMed] [Google Scholar]
  56. Milton I. et al. Age-dependent lethality in novel transgenic mouse models of central nervous system arteriovenous malformations. Stroke 43, 1432–1435, doi: 10.1161/STROKEAHA.111.647024 (2012). [DOI] [PubMed] [Google Scholar]
  57. Soubrier F. et al. Genetics and genomics of pulmonary arterial hypertension. J Am Coll Cardiol 62, D13–D21, doi: 10.1016/j.jacc.2013.10.035 (2013). [DOI] [PubMed] [Google Scholar]
  58. Ojeda-Fernandez L. et al. Reduced plasma levels of Ang-2 and sEng as novel biomarkers in hereditary hemorrhagic telangiectasia (HHT). Clin Chim Acta 411, 494–499, doi: 10.1016/j.cca.2009.12.023 (2010). [DOI] [PubMed] [Google Scholar]
  59. Scholz A., Plate K. H. & Reiss Y. Angiopoietin-2: a multifaceted cytokine that functions in both angiogenesis and inflammation. Ann N Y Acad Sci 1347, 45–51, doi: 10.1111/nyas.12726 (2015). [DOI] [PubMed] [Google Scholar]
  60. Gerald D., Chintharlapalli S., Augustin H. G. & Benjamin L. E. Angiopoietin-2: an attractive target for improved antiangiogenic tumor therapy. Cancer Res 73, 1649–1657, doi: 10.1158/0008-5472.CAN-12-4697 (2013). [DOI] [PubMed] [Google Scholar]
  61. Fischer A., Zalvide J., Faurobert E., Albiges-Rizo C. & Tournier-Lasserve E. Cerebral cavernous malformations: from CCM genes to endothelial cell homeostasis. Trends Mol Med 19, 302–308, doi: 10.1016/j.molmed.2013.02.004 (2013). [DOI] [PubMed] [Google Scholar]
  62. Kim H., Pawlikowska L., Su H. & Young W. L. In Stroke: Pathophysiology, Diagnosis, and Management Vol. 6 (eds Grotta James C. et al.) Genetics and Vascular Biology of Angiogenesis and Vascular Malformations ( Chapter 12). Page 149 (Elsevier, 2015). [Google Scholar]
  63. Pitulescu M. E., Schmidt I., Benedito R. & Adams R. H. Inducible gene targeting in the neonatal vasculature and analysis of retinal angiogenesis in mice. Nat Protoc 5, 1518–1534, doi: 10.1038/nprot.2010.113 (2010). [DOI] [PubMed] [Google Scholar]
  64. Dorff K. C. et al. GobyWeb: simplified management and analysis of gene expression and DNA methylation sequencing data. PLoS One 8, e69666, doi: 10.1371/journal.pone.0069666 (2013). [DOI] [PMC free article] [PubMed] [Google Scholar]
  65. Abecasis G. R. et al. A map of human genome variation from population-scale sequencing. Nature 467, 1061–1073, doi: 10.1038/nature09534 (2010). [DOI] [PMC free article] [PubMed] [Google Scholar]
  66. Dobin A. et al. STAR: ultrafast universal RNA-seq aligner. Bioinformatics 29, 15–21, doi: 10.1093/bioinformatics/bts635 (2013). [DOI] [PMC free article] [PubMed] [Google Scholar]
  67. Campagne F., Dorff K. C., Chambwe N., Robinson J. T. & Mesirov J. P. Compression of structured high-throughput sequencing data. PLoS One 8, e79871, doi: 10.1371/journal.pone.0079871 (2013). [DOI] [PMC free article] [PubMed] [Google Scholar]
  68. Campagne F., Digan W. E. R. & Simi M. MetaR: simple, high-level languages for data analysis with the R ecosystem. bioRxiv, 030254 (2015). [Google Scholar]
  69. Law C. W., Chen Y., Shi W. & Smyth G. K. voom: Precision weights unlock linear model analysis tools for RNA-seq read counts. Genome Biol 15, R29, doi: 10.1186/gb-2014-15-2-r29 (2014). [DOI] [PMC free article] [PubMed] [Google Scholar]
  70. Benjamini Y. & Hochberg Y. Controlling the False Discovery Rate: A Practical and Powerful Approach to Multiple Testing. Journal of the Royal Statistical Society. Series B (Methodological) 57, 289–300 (1995). [Google Scholar]
  71. Livak K. J. & Schmittgen T. D. Analysis of relative gene expression data using real-time quantitative PCR and the 2(-Delta Delta C(T)) Method. Methods 25, 402–408, doi: 10.1006/meth.2001.1262 (2001). [DOI] [PubMed] [Google Scholar]
  72. Chatterjee P. K., Al-Abed Y., Sherry B. & Metz C. N. Cholinergic agonists regulate JAK2/STAT3 signaling to suppress endothelial cell activation. Am J Physiol Cell Physiol 297, C1294–C1306, doi: 10.1152/ajpcell.00160.2009 (2009). [DOI] [PMC free article] [PubMed] [Google Scholar]
  73. Vingtdeux V. et al. CALHM1 ion channel elicits amyloid-β clearance by insulin-degrading enzyme in cell lines and in vivo in the mouse brain. J Cell Sci 128, 2330–2338, doi: 10.1242/jcs.167270 (2015). [DOI] [PMC free article] [PubMed] [Google Scholar]

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Supplementary Materials

Supplementary Information
srep37366-s1.xls (87KB, xls)
Supplementary Information
srep37366-s2.pdf (4.7MB, pdf)

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