Open access peer-reviewed chapter

TGF-β Activation and Signaling in Angiogenesis

Written By

Paola A. Guerrero and Joseph H. McCarty

Submitted: 09 June 2016 Reviewed: 19 October 2016 Published: 05 April 2017

DOI: 10.5772/66405

From the Edited Volume

Physiologic and Pathologic Angiogenesis - Signaling Mechanisms and Targeted Therapy

Edited by Dan Simionescu and Agneta Simionescu

Chapter metrics overview

3,246 Chapter Downloads

View Full Metrics


The transforming growth factor-β (TGF-β) signaling pathway regulates various cellular processes during tissue and organ development and homeostasis. Deregulation of the expression and/or functions of TGF-β ligands, receptors or their intracellular signaling components leads to multiple diseases including vascular pathologies, autoimmune disorders, fibrosis and cancer. In vascular development, physiology and disease TGF-β signaling can have angiogenic and angiostatic properties, depending on expression levels and the tissue context. The objective of this chapter is to analyze the mechanisms that contribute to the activation and signaling of TGF-β in developmental, physiological and pathological angiogenesis, with a particular emphasis on the importance of TGF-β signaling in the mammalian central nervous system (CNS).


  • TGF-β
  • vasculogenesis
  • angiogenesis
  • VEGF

1. Introduction

Discovery of TGF-βs was the result of independent efforts by several laboratories [14] during characterization of a secreted factor from fibroblasts transformed by the Moloney sarcoma virus (MSV). The TGF-β superfamily is now known to be composed of more than 30 chemokines such as TGF-β1-β3, activins, anti-Müllerian hormone (AMH), bone morphogenetic proteins (BMPs), growth and differentiation factors (GDFs) and NODAL that can signal via canonical and noncanonical receptors and intracellular effector proteins [5].

The best characterized member of the TGF-β family, TGF-β1, is initially produced from a single gene as a large precursor known as pre- and pro-TGF-βs which undergo two proteolytic cleavage events. The first signal peptide is cleaved in the rough endoplasmic reticulum. Furin, a proprotein convertase, subsequently cleaves the protein into two fragments [6]. The carboxy terminus corresponds to the functionally active cytokine and the large amino terminus is latency-associated protein (LAP), also referred to as the prodomain. Regardless of this processing by furin, the mature and LAP domains remain associated by noncovalent bonds to form the small latent complex (SLC). This complex subsequently covalently interacts with a second gene product, the latent TGF-β binding protein (LTBP), and is incorporated into a larger latent complex (LLC) that associates with the extracellular matrix (ECM) [6]. Three-dimensional crystal structure of porcine latent TGF-β1 shows a conformation that resembles a ring-like shape [7]. Two domains were defined in the structure: (i) an arm domain that contains an integrin-binding Arg-Gly-Asp (RGD) peptide motif and (ii) a “straitjacket” domain where the mature TGF-β is encased. At the opposite end of the arm domain, LTBP binds the prodomain forming the “ring head” [7] (Figure 1).

Figure 1.

TGF-β processing and activation. (a)TGF-β precursor undergoes proteolysis at its N-terminus (black arrow head) which results in the removal of its signal peptide. (b)In a second proteolytic cleavage event by furin (blue arrow head), the precursor is separated into a large LAP or prodomain (gray) and the mature TGF-β (red) and (c)Schematic view of the closed ring structure (left) and unfastened straitjacket (right) conformation corresponding to the inactive LAP-TGF-β and mature TGF-β, respectively.

After secretion, the LLC complex interacts with various ECM proteins, such as fibronectin and fibrillin, and is maintained in an inactivated form [8]. TGF-β is activated by different mechanisms, including interactions with integrins, alterations in pH and extracellular proteases. αν integrin, which forms heterodimers with five different β integrin subunits (β1, β3, β5, β6 and β8), that bind to LAP-TGF-β1 and LAP-TGFβ-3 [9, 10]. However, only ανβ6 and ανβ8 have been shown to activate the latent TGF-β complex [11]. Activation by both ανβ6 and ανβ8 integrins requires the RGD motif in LAP. Activation by ανB6 requires an intact cytoplasmic domain [12, 13] and the presence of other ECM proteins [14]. Activation by ανβ8, however, does not require the integrin cytoplasmic domain, but it is reported to require the presence of metalloproteinases (MMPs) on the cell surface or in the ECM [9]. Additionally, in T cells, ανβ6 and ανβ8 can activate LAP-TGF-β in cooperation with the glycoprotein-A repetitions predominant protein (GARP) [15, 16].

TGF-β is also activated by proteases. Aspartyl (e.g., cathepsin D) [17], cysteine (e.g., calpain) [18] and serine proteases (e.g., plasmin and kallikreins) and metalloproteases have shown to stimulate the release of chemokine from the latent complex, although most of these studies have been performed in vitro [19]. Moreover, TGF-β has been reported to be activated by other nonprotease mechanisms such as neuropilin1 (Nrp1), thrombospondin (TSP-1), F-spondin, pregnancy-specific beta-1-glycoprotein 1 (PSG1) and deglycosylation. Likewise, there are chemical and physical settings that activate TGF-β, for example, heat, ultraviolet radiation, physical shear, detergents and reactive oxygen species [8].

Three-dimensional structural studies of the LLC reveal that the RGD motifs are readily available for integrin engagement. Hydrophobic side chains, which have been identified near the RGD motif, likely enhance integrin binding [7]. In the presence of ανβ6, LLC can bind one or two integrin monomers. However, this binding does not induce required conformational changes to promote the complete activation of TGF-β, which is in agreement with prior mutational studies [12, 13, 20]. Furthermore, in accord with previous studies, the crystal structure of latent TGF-β predicts that pulling forces, emanating from the integrin C-terminal cytoplasmic tail that interacts with the cytoskeleton and binding RGD via the N-terminal extracellular region, are counteracted by associations with the ECM. Therefore, in the latent TGF-β, the straitjacket domain is maintained in a closed conformation until tensile forces are applied from both ends of the structure, resulting in loosening of the straitjacket domain and the release of the mature TGF-β. This study also showed that an additional feature of the prodomain is to prevent access to activating receptors [7].


2. TGF-β signaling pathways

Signaling is regulated by three major receptors: TGF-β receptor type I (TβRI), type II (TβRII) and type III (TβRIII). In general, TGF-β binds TβRIII, which facilitates its delivery to TβRII, a constitutively active kinase, leading to the subsequent phosphorylation and activation of TβRI. In humans, there are seven TβRIs, also known as activin receptor-like kinases (ALK), and five TβRIIs [5]. In most cells, ALK-5 forms a heterodimer with TβRII bound to TGF-β, which activates the ALK-5 kinase domain via phosphorylation of its GS domain. This receptor activation propagates intracellular signaling through ‘canonical’ effector proteins mothers against decapentaplegic homolog 2/SMAD family member 2 (Smad2) and Smad3, which are transcription factors. Once phosphorylated, these Smad proteins form a complex with Smad4 leading to nuclear translocation and initiation of genes transcription. In most normal cells, TGF-β-mediated activation of Smads leads to inhibition of cell growth. More specifically, the Smad2/3-4 complex partners with foxhead box O (FOXO) factors to activate p21Cip1 (CDKN1A), which inhibits cyclin-dependent kinase 1(CDK1), resulting in cell cycle arrest. Similarly, TGF-β can also activate p15Inkab (CDKN2B), the CDK4 inhibitor, through the SMAD2-3/4-FOXO1 axis (Figure 2) [5].

Figure 2.

TGF-β canonical pathway. (a)In normal cells and early stages of cancer TGF-β promotes cell cycle arrest. Repressors of the pathway are shown in red. Blue dots represent protein phosphorylation and (b)in endothelial cells, an alternative pathway promotes cell proliferation.

Likewise, TGF-β acts as a cytostatic factor by decreasing c-Myc expression and downregulating the inhibitor of DNA-binding protein (ID) 1 and ID3 transcription factors. ID1 and ID3 are involved in differentiation, cell cycle progression and self-renewal of stem cells [21, 22]. TGF-β elicits c- Flk-1myc repression by promoting SMAD3 binding to a repressing Smad-binding element (RSBE) at the c-myc promoter [23]. c-Myc can be recruited to the promoters of CDKN1A and CDKN2B by the Myc-interacting zinc-finger (MIZ-1). This blocks CDK expression and results in apoptosis [24]. Additionally, in endothelial cells (ECs), TGF-β can target a second receptor type 1, ALK-1, which signals through Smad1/5/8 and stimulates angiogenic factors, such as interleukin 1 receptor-like 1 and ID1 (Figure 2) [25].

Several proteins are known to antagonize canonical TGF-β signaling. For example, (i) PI3K activates AKT which phosphorylates the SMADs-FOXO complex and inhibits its translocation to the nucleus [21], (ii) foxhead box G1 (FOXG1) inhibits the SMADs-FOXO complex [21], (iii) SMAD7 can trigger TβRI for proteosomal degradation by recruiting SMAD-specific E3 ubiquitin protein ligase (SMURF1) and SMURF2 [26], (iv) SMAD6 blocks SMAD1 through SMAD4 binding, (v) Erk proteins phosphorylate SMADs and inhibit their nuclear translocation, (vi) BAMBI, a pseudoreceptor, dimerizes with TβRI leading to its inactivation, (vii) FKBP12 binds to TβRI and impedes its phosphorylation, activation and signaling [27] and (viii) protein arginine N-methyltransferase 1 (PRMT1) methylates SMAD6 and allows BMP signaling through SMADs1/5 [2830].


3. Vasculogenesis

During embryogenesis, the development of the vascular system is divided into three stages, vasculogenesis, angiogenesis and arteriogenesis. Vasculogenesis occurs in embryonic organs as well as extraembryonic tissues such as the placenta, yolk sac and allantois [31]. The earliest discernible structures in vasculogenesis, the blood islands, are formed in the mouse yolk sac by embryonic day (E) 6.5–7. This structure contains precursor cells or hemangioblasts, which differentiate to EC and hematopoietic cells [32]. At E8.5, cells located toward the periphery of the blood island, or angioblasts, differentiate into EC, while cells located toward the central region give rise to hematopoietic precursor cells. Next, lumenization takes place; tight junctions and basement membranes develop, and pericytes are recruited to blood vessels and promote maturation [33].

Several growth factors have been identified to regulate vasculogenesis, such as vascular endothelial growth factor (VEGF), fibroblast growth factor (FGF), the hedgehog family, neuropilins, integrins, fibronectin and TGF-βs. FGF-2 has been reported to participate in the generation of the angioblast in quail/chick chimeras and in vessel formation [34].

Hedgehog signaling has been shown to be crucial in the initial steps of vasculogenesis. It promotes differentiation of the primitive endoderm into both, endothelial and hematopoietic lineage [35]. For instance, blocking Indian hedgehog (Ihh) causes signaling repression from the visceral ectoderm and consequently abrogation of vasculogenesis and hematopoiesis in anterior epiblast [35]. Deletion of Ihh in mouse caused 50% lethality at midgestation with the remaining 50% dying at birth. Defects in blood vessel formation have been proposed as the cause for the lethality, which has been supported by experiments showing: (i) deletion of Sonic hedgehog (Shh) in mice resulted in a reduction in vascularization in lung [36], (ii) overexpression of Shh resulted in an increase in vascularization in neuroectoderm [37], (iii) depletion of Shh in zebrafish caused defective vasculature [38] and (iv) depletion of Ihh from stem cell-derived embroid bodies inhibited blood island differentiation [39].

VEGF signaling is crucial in vasculogenesis. Genetic studies have shown that deletion of Flt-1 (VEGFR1), Flk-1/KDR (VEGFR2) and one or both alleles of VEGF cause embryonic lethality. VEGFR1 mutants exhibit aberrant central localization of the angioblasts in the blood island, instead of their normal localization toward the periphery [40]. These results implied that the growth of ECs was not inhibited in this region and led to the idea that VEGR1 hampers signaling from VEGF by ligand sequestration [33]. In addition, VEGFR2 mutants die around E9. In these embryos, both vasculogenesis and hematopoiesis do not initiate which was explained by faulty blood island in which cell migration was abrogated [41, 42]. Similarly, mutant heterozygous for VEGF die by E11 and showed impaired vasculogenesis and angiogenesis. These embryos showed severe abnormalities, such as underdeveloped brain and heart, decreased number of nucleated red blood cells in blood islands and aberrant vasculature in nervous system and placenta [43].

Neuropilins are co-receptors for VEGF receptors. Nrp1 is found in ECs of arteries, while neuropilin 2 (Nrp2) is found at the endothelium of lymphatic vessels and veins. Deletion of Nrp1 in mice affects severely the central and peripheral nervous systems, as well as the yolk sac vasculature [44]. In contrast, depletion of Nrp2 has no effects in the vasculature of arteries or veins, but it does affect angiogenesis of the lymphatic vasculature [45, 46]. In addition, mice harboring deletions in both neuropilins have shown obstruction in vasculogenesis in the yolk sac and in the formation of the primary vascular plexus [47].


4. Developmental angiogenesis

Angiogenesis is the formation of new blood vessels from existing vasculature. It occurs by mechanisms including sprouting angiogenesis and intussusceptive angiogenesis (Figure 3). Sprouting angiogenesis initiates with the selection of endothelial tip cells at the vessel wall. These cells react toward extracellular stimuli and secrete proteolytic enzymes to digest the surrounding ECM. Tip cells are connected to endothelial stalk cells to direct the vascular sprout [33, 48, 49]. Once the new tube is formed and a lumen is established, the vessel is stabilized by the recruitment of pericytes to capillaries or vascular smooth muscle cells (vSMC) to arteries and veins [6, 33], leading to re-establishment of mature blood vessels.

Figure 3.

Mechanisms of angiogenesis. (a)Sprouting and (b)intussusceptive angiogenesis.

Intussusceptive angiogenesis, also known as splitting angiogenesis, results in the formation of intermediate intracapillary pillars. This mechanism is more efficient than sprouting angiogenesis since it does not require cell proliferation. Instead, it needs the reorganization of existing ECs. In this process, (i) ECs from opposite sides of the blood vessel make contacts, (ii) ECs from both ends reorganize and cause a splitting in the vessel wall, (iii) an interstitial pillar core is generated and (iv) myofibroblasts, pericytes and finally collagen invade the pillar and a basement membrane is formed [33, 49, 50].


5. TGF-β in vasculogenesis and angiogenesis

5.1. Mutant phenotypes in mice lacking components of the TGF-B pathway

TGF-β mRNA was initially detected by PCR in preimplantation stages and in situ expression was present as early as E7.5, suggesting important roles in early development [51, 52]. In the embryo, proper TGF-β was detected in angioblast progenitors within the primitive heart mesoderm. Likewise, its expression was detected in extraembryonic tissues, including in the allantois mesoderm, and within blood islands of the yolk sac [53].

Deletion of the TGF-β1 gene in mice resulted in 50% lethality in utero, with the remaining 50% of mutant mice surviving up to three weeks postnatally. Histopathology analyses showed multifocal inflammatory cell infiltration and necrosis in several organs, especially the heart and stomach [53, 54]. It was subsequently shown that maternal contributions of TGFB1 RNA and other genetic and epigenetic factors contributed to 50% postnatal survival [55].

The 50% of TGF-β mutants showed lethality and resorption by E10.5. Analysis of E8.5 embryos did not show significant morphological defects. However, analysis of E9.5 and E10.5 embryos resulted in a range of phenotypic defects within the yolk sac. While in some cases, vasculogenesis was delayed; in other cases, a dramatic reduction in size was observed and it was accompanied by weak and disorganized primary vessels, with some areas displaying complete vessel depletion. Analysis of the yolk sac vasculature indicated that the defects occurred during differentiation of ECs and hematopoietic cells. In contrast, the initial differentiation of mesodermal cells into ECs was not affected [52].

Genetic ablation of TβRII resulted in very similar phenotypes as in TGF-β1 mutants, with alterations in yolk sac vasculature and embryonic lethality by E10.5- E11.5 [56]. Mutants in endoglin also showed defects in vascular vessels within and outside the embryo. Embryo lethality was observed at E11.5, with mutants developing focal hemorrhage [57, 58]. Similarly, engineered mutations in mice that abrogate the expression of ALK1, ALK5, SMAD1 or SMAD5 resulted in defects in cardiovascular development [57, 59, 60].

5.2. Roles of TGF-β in angiogenesis

Early work to determine the roles for TGF-βs in ECs was contradictory. TGF-β signaling was initially found to inhibit cell migration and proliferation [61, 62], yet later studies indicated that it promotes cell proliferation [6366]. The relative levels of expression of TGF-β seem to partially explain these discrepancies, with low doses promoting angiogenesis and higher levels resulting in growth inhibition of ECs and maturation of blood vessels [66, 67]. For instance, during blood vessel coverage by smooth muscle cells, TGF-β paracrine signaling from ECs to mesenchymal cells results in vascular smooth muscle cell and pericyte differentiation [6].

TGF-β also plays a role in the angiogenic process of hypoxic tissue. For instance, during infarction (stroke), neovascularization occurs primarily at the ischemic penumbra (periphery of the infarct), which correlates with high levels of both mRNA and active TGF-β protein [68]. Similarly, during organ transplant VEGF and TGF-β1, levels are increased in devascularized hypoxic tissue. TGF-β3 was also upregulated in hypoxic tissues, but to a lesser degree [69].

TGF-β regulates angiogenesis by different mechanisms; for example, it is involved in vessel proliferation and maturation by alternating two signaling cascades with opposite effects (ALK1 and ALK5). Likewise, TGF-β can promote its own expression, and it upregulates the expression of other angiogenic factors such as, platelet-derived growth factor (PDGF), interleukine-1, basic fibroblast growth factor (bFGF), tumor necrosis factor alpha and transforming growth factor alpha [70]. TGF-β can change the functions of other factors, such as VEGF, from prosurvival to pro-apoptotic [71]. Similarly, in vitro work has shown that in ECs TGF-β upregulates the expression of endothelin (EDN1), PDGFA and PDGFB, nitric oxide synthase 3 (NOS3), actin, alpha 2, smooth muscle, aorta (ACTA2), secreted protein acidic and cysteine rich (SPARC), TSP-1, fibronectin (FN1), collagens (COL1A1, COL4A1, and COL5A1), plasminogen activator (PLAU), serpin family E member 1 (SERPINE1) and integrins (ITGB1, ITGB3, ITGAV, ITGA2 and ITGA5). It can also downregulate several genes, such as selectin-E (SELE), KDR, von Willebrand factor (VWR), thrombomodulin (THBD), monocyte chemo-attractant protein (MCP1), C-X-C motif chemokine ligand 1 (CXCL1), integrins (ITGB1, ITGB3, ITGA5 and ITGA6), TIMP1 and PLAU [70].

Levels of ALK1 and ALK5 determine TGF-β mitogenic or mitostatic responses in ECs. ALK5-Smad2/3 signaling stimulates transcription of ECM proteins such as fibronectin and plasminogen activator inhibitor type 1, which promote the resolution of angiogenesis by inducing vessel maturation. In contrast, signaling via the ALK1-Smad1/5/8 pathway generates anti-angiogenic responses [25, 51]. This requires a TGF-β accessory receptor, endoglin, which enhances ALK1 signaling and inhibits ALK5 cytostatic phenotype [72]. More recent work has shown that in the mouse eye retina the leucine-rich alpha-2-glycoprotein (Lrg1), which binds endoglin, promotes angiogenesis through Alk1-Smad1/5/8 in the presence of TGF-β [73].

5.2.1. TGF-β signaling in CNS development

In the mammalian CNS, neurons, astrocytes, pericytes and ECs closely interact to form a multicellular neurovascular unit [11]. During embryonic brain development, TGF-β is critical for sprouting angiogenesis of the CNS. In particular, TGF-β has been shown to work in conjunction with αν integrins to regulate paracrine signaling between neuroepithelial cells and ECs within neurovascular units. In mouse, embryos deletion of αν integrin showed vascular defects that were restricted mainly to the brain. This phenotype was recapitulated in β8 integrin mutant embryos. In contrast, deletion of β3 and β5 integrins did not cause brain vasculature abnormalities [74, 75]. Cell type-specific deletion of αν and β8 integrins in nervous system glial cells resulted in developmental intracerebral hemorrhage as well as postnatal motor dysfunction and seizures. Of note, the brain hemorrhage observed in embryos was absence in adult mice, suggesting that a compensatory mechanism that repairs hemorrhage occurs after birth [75, 76]. Interestingly, αν ablation in vascular ECs did not show a phenotype [75]. In later work, in which an outbred background was used to overcome the effects of β8−/− embryonic lethality, it was shown that adult mice lacking β8 integrin displayed neurovascular pathologies [77]. Most notably, adult β8 integrin mutants displayed a reduction in olfactory bulb size and abnormalities at the subventricular zone and rostral migratory stream. Neuroblasts generated in the subventricular zone utilize blood vessels as guides to migrate within the rostral migratory stream and differentiated to neurons within the olfactory bulbs. The size-reduced olfactory bulbs in adult β8−/− mice revealed essential roles for this integrin in promoting neuroblast migration along blood vessels. These defects correlated with a reduction in TGF-β signaling in neurospheres dissected from β8−/− mice [77].

The brain vascular defects observed in Itgb8 null mutants are also shared by Tgfb1 and Tgfb3 loss of function mutants. In addition, mutating the integrin-binding RGD binding site in Tgfb1 leads to early embryonic lethality [78]. Similarly, mice lacking both β6 and β8 integrins showed similar phenotypes as null mutants for Tgfb1 and Tgfb3 [78].

More recently, integrin β8 and Nrp1 have been shown to mediate neuroepithelial-endothelial cell interactions. β8 integrin in the neuroepithelium activates TGF-β signaling in ECs, while Nrp1 suppresses canonical TGF-β signaling, thus controlling normal sprouting angiogenesis [79]. Disruption of TGF-β signaling by targeting β8 integrin or Nrp1 results in excessive vessels sprouting and branching and formation of dysplastic glomeruloid-like vessels that are hemorrhagic [80].

The ανβ8-TGF-β connection in developmental angiogenesis in the brain also regulated neovascularization in the developing retina, where β8 integrin is expressed in astrocytes and Muller glial cells, a neuroepithelial cell type specifically found in the retina [81]. β8−/− retinas display abnormalities in the formation of the secondary vascular plexus, including impaired sprouting and formation of blood vessels with glomeruloid-like tufts. In addition, intraretinal hemorrhage was detected [81]. Furthermore, ablation of αν or β8 integrins but not of Tgfbr2 in astrocytes resulted in defects in angiogenesis, and blocking TGF-β1 with neutralizing antibodies affected paracrine signaling to ECs [81]. This work was confirmed later in a study showing that Tgfbr2 deletion in ECs of neonatal mice caused bleeding in the brain and vascular abnormalities, hemorrhage and deficiency in the formation of the deeper vascular network in the retina [82, 83]. Similarly, reduced Smad2 phosphorylation was observed in ECs from retina of Tgfbr2 knockout mice [82].


6. TGF-β in pathological angiogenesis

Genetic mutations in TGF-β signaling components are associated with various human vascular pathologies. For example, mutations in the TβRIII/endoglin gene are linked to hereditary hemorrhagic telangiectasia (HHT) and Osler-Rendu-Weber syndrome. The disease is characterized, among others, by arteriovenous malformations (AVM) in the liver, brain and lung, telangiectases in skin and mucous membranes and recurrent epistaxis [84]. In trying to understand AVM, it was proposed that TGF-β paracrine signaling from ECs to vascular smooth muscle cells and/or pericytes was reduced. As a consequence, vascular smooth muscle cell differentiation was affected and this resulted in fragile, leaky blood vessels [85]. Alternatively, other suggested mechanisms underlying AVM endothelial cell apoptosis and depletion of smooth muscle cells [6]. In addition, it was discovered that brain AVM present decreased levels of integrin β8 which correlates with decreased TGF-β activation and signaling in ECs [86]. Mutations in human ITGAV and ITGB8 genes also predispose some families to spontaneous brain hemorrhage [87].

In cancer, angiogenesis is not properly regulated as it occurs in developmental and physiological settings. Hypoxic conditions and proangiogenic factors released by tumor cells promote robust new blood vessel formation. The intratumoral vasculature is often disorganized and leaky with hypertension and acidosis. Similarly, tumor ECs display aneuploidy as well as centrosome and chromosomal amplifications [88]. The TGF-β pathway is affected by either mutations in the main signaling components, in particular SMADs, or by altered expression of repressive factors (e.g., FOXG1, PI3K-AKT and C-MYC) (Figure 1). Analysis of copy number alterations using data from The Center Genome Atlas (TCGA) and analyzed by cBioportal show that Smad2, 3 and 4 are mutated, deleted or amplified in several tumor types, but especially in pancreatic, colorectal and gastric cancers [89, 90].

During tumor growth and progression, TGF-β plays a dual role as both an angiogenic and angiostatic factor [6]. In early-stage tumors, higher TGF-β expression levels are correlative with a better prognosis. TGF-βs exert cell cycle arrest by downregulating c-Myc and Ids 1–3 in late G1 phase and by promoting the expression of cyclin-dependent protein kinase inhibitors [25]. As a proangiogenic factor, TGF-β pathway collaborates with VEGF, PDGF and bFGF in autocrine/paracrine signaling. In highly vascularized tumors, such as GBM and hepatocellular carcinoma (HCC), TGF-β levels are upregulated. In HCC cells, TGF-β induces the secretion of VEGF-A. Accordingly, inhibition of TGF-β by the TβRI/II synthetic kinase inhibitor LY2109761 showed decreased tumor size, vessel density and VEGF expression. This inhibitor also affected paracrine signaling between tumor cells and ECs. These effects on VEGF-A were dependent on SMAD2/3 expression levels [91]. Likewise, TGF-β inhibition in other cancer types such as colorectal cancer and GBM has also led to reduce intratumoral vascularization [59, 9294]. Of note, the increase in angiogenesis caused by TGF-β in GBM was decreased by inhibition of the JNK pathway [95]. TGF-β family members also promote the secretion of MCP1 and TGF-α [96, 97], which impact inflammatory cells in the tumor microenvironment.

6.1. VEGF regulation by TGF-β

TGF-β promotes the expression of a major regulator of vasculogenesis and angiogenesis, VEGF. The VEGF family is comprised of a large group of secreted glycoproteins that interact with various cell surface receptors. VEGF-A is expressed as four different isoforms (121, 165, 189, 206 a.a.). Isoform 121 has low binding for heparan sulfate and diffuses away from its secreted location creating a chemogradient. Isoform 165 has higher affinity to heparan sulfate compared with 121, and it shows the highest mitogenic capacity among all isoforms. Finally, isoforms 189 and 206 have shown the highest binding capacity to bind heparan sulfates and are known to interact with other components of the ECM [33]. These ligands bind mainly three tyrosine kinase receptors (VEGFR) 1–3. VEGF-A has been a major therapeutic target in cancer due to its upregulation in many cancer types. Unfortunately, anti-angiogenic therapies that target VEGF-A, such as the neutralizing antibody Bevacizumab, have been unsuccessful in clinical studies where patients have shown resistance to anti-VEGF therapy. Similarly, in vitro studies performed in GBM cell lines indicated that irradiation enhances VEGF secretion [98101].

FGF-2 induces VEGF expression in ECs via paracrine and autocrine signaling mechanisms [71]. TGF-β balances FGF-2 by suppressing the induction of plasminogen activator, a serine protease involved in the migration of cells, which is required in the formation of capillaries during angiogenesis [102]. In contrast, TGF-β induces ECs apoptosis as part of capillary remodeling and at the same time promotes ECs expression of VEGF [103]. VEGF-A is an ECs survival factor and protects ECs from apoptosis [104]. More recent work has shown that VEGF targets p38MAPK resulting in ECs survival. In contrast, in the presence of TGF-β, FGF-2 is activated, promoting VEGF upregulation, p38MAPK activation and apoptosis [71].

6.2. Upregulation of TGF-β in GBM

In GBM, an “angiogenic switch” marks the transition from low to more malignant tumors where ECs proliferate, resulting in a major increase in blood vessels. This excessive growth in vasculature was initially thought to be required for maintaining the aggressive growth rate of GBM. However, recent work suggests that these aberrant blood vessels are also required to maintain glioma stem cells (GSC), which are known to localize in close proximity to ECs in a perivascular niche. These cells secrete VEGF and express VEGFR2, and this complex is stabilized by NRP1. This axis is involved in the self-renewal, survival and tumorigenic capacity of GSCs [105]. Recent work has shown that TGF-β induces differentiation of GSCs into pericytes to support vessel formation and tumor growth [106].

TGF-β cooperates in glioma angiogenesis by enhancing the expression of FGF, VEGF, PDGF-β, and CD44. Increased expression of FGF promotes VEGF expression. High levels of TGF-β in gliomas correlate with poor prognosis, and it is known to work in conjunction with the PDGF-β to increase GSCs proliferation [107]. In vSMC, TGF-β expression increases the levels of PDGF-β, its receptor (βPDGFR) and of EGF receptor (EGFR). βPDGFR promotes VEGF expression and secretion in ECs and signals through PI3K [108].

Angiogenesis in GBM develops by two mechanisms: microvascular cell proliferation and sprouting. The origin of microvascular proliferation seems to arise from hypoxia, where cells migrate away from the hypoxic center as a result of an increase in the levels of migration-related genes. As a consequence, the center becomes necrotic and the cells surrounding it form a palisade, which secretes angiogenic factors such as VEGF. This promotes neighboring angiogenesis, known as glomeruloid-like microvascular proliferation, composed of both endothelial and smooth muscle cells. In contrast, the increase in angiogenic capillaries can be observed by staining with markers such as CD31 and Factor VIII-related antigen (Figure 4) [109].

Figure 4.

Microvascular proliferation. (a)Hypoxia center, (b)cell migration, (c)necrosis (N) and (d)glomeruloid microvascular proliferation (arrow heads).

TGF-β1-3 levels and endoglin-ALK1 signaling are elevated under hypoxic conditions. In addition, under hypoxia, Snail and Slug expression levels are increased. These genes are known to be involved in endothelial to mesenchymal transition and in sprouting angiogenesis and are regulated by TGF-β in ECs [110].

Integrins are important activators of the TGF-β pathway. They are important in regulating tumor angiogenesis by serving as receptors for ECM components, such as laminin, tenascin, fibronectin and collagens [111]. ανβ3 is a receptor for various secreted ECM proteins, such as von Willebrand factor, TSP-1, fibrinogen, proteolyzed collagen, fibronectin and vitronectin, and it is involved in angiogenesis and vascular remodeling. For instance, ανβ3 integrin associates with MMP-2 in blood vessels of melanoma tumors, and this binding facilitates collagen degradation in vitro [112]. In GBM, TGF-β enhances ανβ3 integrin adhesion and expression and promotes integrin-mediated motility [111].

ανβ8 is expressed in GBM cell lines and primary tumors samples. GBM cell lines overexpressing ανβ8 show an increase in proliferation but when injected into the brain generate tumors with a decrease in vascularity. Silencing αν or β8 integrin in transformed astrocytes or in human GBM cell lines leads to decreased in TGF-β signaling, resulting in increased tumor size, intratumoral hemorrhage and decreased tumor cell invasiveness [113, 114].

In summary, TGF-β signaling is a crucial pathway in the angiogenesis of normal and tumor cells facilitating interactions between endothelial and epithelial cells. The vast majority of research has been focused on the activation of TGF-β, but more work is necessary to understand how the pathway is repressed. This could help to move forward current therapeutic attempts to target components of the TGF-β signaling pathway.


  1. 1. de Larco JE, Todaro GJ. Growth factors from murine sarcoma virus-transformed cells. Proceedings of the National Academy of Sciences of the United States of America. 1978;75(8):4001–5.
  2. 2. Moses HL, Branum EL, Proper JA, Robinson RA. Transforming growth factor production by chemically transformed cells. Cancer Research. 1981;41(7):2842–8.
  3. 3. Roberts AB, Anzano MA, Lamb LC, Smith JM, Sporn MB. New class of transforming growth factors potentiated by epidermal growth factor: isolation from non-neoplastic tissues. Proceedings of the National Academy of Sciences of the United States of America. 1981;78(9):5339–43.
  4. 4. Moses HL, Roberts AB, Derynch R. The Discovery and Early Days of TGF-B: A Historical Perspective. Cold Spring Harbor Perspectives in Biology. 2016; 8(7): pii: a021865.
  5. 5. Massague J. TGFbeta signalling in context. Nature Reviews Molecular Cell Biology. 2012;13(10):616–30.
  6. 6. ten Dijke P, Arthur HM. Extracellular control of TGFbeta signalling in vascular development and disease. Nature Reviews Molecular Cell Biology. 2007;8(11):857–69.
  7. 7. Shi M, Zhu J, Wang R, Chen X, Mi L, Walz T, et al. Latent TGF-beta structure and activation. Nature. 2011;474(7351):343–9.
  8. 8. Robertson IB, Rifkin DB. Regulation of the bioavailability of TGF-beta and TGF-beta related proteins. Cold Spring Harbor Perspectives in Biology. 2016;8(6).pii: a021907
  9. 9. Mu D, Cambier S, Fjellbirkeland L, Baron JL, Munger JS, Kawakatsu H, et al. The integrin alpha(v)beta8 mediates epithelial homeostasis through MT1-MMP-dependent activation of TGF-beta1. Journal of Cell Biology. 2002;157(3):493–507.
  10. 10. Ludbrook SB, Barry ST, Delves CJ, Horgan CM. The integrin alphavbeta3 is a receptor for the latency-associated peptides of transforming growth factors beta1 and beta3. Biochemical Journal. 2003;369(Pt 2):311–8.
  11. 11. McCarty JH. Integrin-mediated regulation of neurovascular development, physiology and disease. Cell Adhesion & Migration. 2009;3(2):211–5.
  12. 12. Munger JS, Huang X, Kawakatsu H, Griffiths MJ, Dalton SL, Wu J, et al. The integrin alpha v beta 6 binds and activates latent TGF beta 1: a mechanism for regulating pulmonary inflammation and fibrosis. Cell. 1999;96(3):319–28.
  13. 13. Annes JP, Chen Y, Munger JS, Rifkin DB. Integrin alphaVbeta6-mediated activation of latent TGF-beta requires the latent TGF-beta binding protein-1. Journal of Cell Biology. 2004;165(5):723–34.
  14. 14. Fontana L, Chen Y, Prijatelj P, Sakai T, Fassler R, Sakai LY, et al. Fibronectin is required for integrin alphavbeta6-mediated activation of latent TGF-beta complexes containing LTBP-1. FASEB Journal: Official Publication of the Federation of American Societies for Experimental Biology. 2005;19(13):1798–808.
  15. 15. Wang R, Zhu J, Dong X, Shi M, Lu C, Springer TA. GARP regulates the bioavailability and activation of TGFbeta. Molecular Biology of the Cell. 2012;23(6):1129–39.
  16. 16. Edwards JP, Thornton AM, Shevach EM. Release of active TGF-beta1 from the latent TGF-beta1/GARP complex on T regulatory cells is mediated by integrin beta8. Journal of Immunology. 2014;193(6):2843–9.
  17. 17. Lyons RM, Keski-Oja J, Moses HL. Proteolytic activation of latent transforming growth factor-beta from fibroblast-conditioned medium. Journal of Cell Biology. 1988;106(5):1659–65.
  18. 18. Abe M, Oda N, Sato Y. Cell-associated activation of latent transforming growth factor-beta by calpain. Journal of Cellular Physiology. 1998;174(2):186–93.
  19. 19. Maeda S, Dean DD, Gay I, Schwartz Z, Boyan BD. Activation of latent transforming growth factor beta1 by stromelysin 1 in extracts of growth plate chondrocyte-derived matrix vesicles. Journal of Bone and Mineral Research: The Official Journal of the American Society for Bone and Mineral Research. 2001;16(7):1281–90.
  20. 20. Wipff PJ, Hinz B. Integrins and the activation of latent transforming growth factor beta1—an intimate relationship. European Journal of Cell Biology. 2008;87(8–9):601–15.
  21. 21. Seoane J, Le HV, Shen L, Anderson SA, Massague J. Integration of Smad and forkhead pathways in the control of neuroepithelial and glioblastoma cell proliferation. Cell. 2004;117(2):211–23.
  22. 22. Anido J, Saez-Borderias A, Gonzalez-Junca A, Rodon L, Folch G, Carmona MA, et al. TGF-beta receptor inhibitors target the CD44(high)/Id1(high) glioma-initiating cell population in human glioblastoma. Cancer Cell. 2010;18(6):655–68.
  23. 23. Frederick JP, Liberati NT, Waddell DS, Shi Y, Wang XF. Transforming growth factor beta-mediated transcriptional repression of c-myc is dependent on direct binding of Smad3 to a novel repressive Smad binding element. Molecular and Cellular Biology. 2004;24(6):2546–59.
  24. 24. Seoane J, Le HV, Massague J. Myc suppression of the p21(Cip1) Cdk inhibitor influences the outcome of the p53 response to DNA damage. Nature. 2002;419(6908):729–34.
  25. 25. Tian M, Neil JR, Schiemann WP. Transforming growth factor-beta and the hallmarks of cancer. Cellular Signalling. 2011;23(6):951–62.
  26. 26. Yan X, Liu Z, Chen Y. Regulation of TGF-beta signaling by Smad7. Acta Biochimica et Biophysica Sinica. 2009;41(4):263–72.
  27. 27. Massague J, Wotton D. Transcriptional control by the TGF-beta/Smad signaling system. EMBO Journal. 2000;19(8):1745–54.
  28. 28. Xu J, Derynck R. Does Smad6 methylation control BMP signaling in cancer? Cell Cycle. 2014;13(8):1209–10.
  29. 29. Xu J, Wang AH, Oses-Prieto J, Makhijani K, Katsuno Y, Pei M, et al. Arginine methylation initiates BMP-induced Smad signaling. Molecular Cell. 2013;51(1):5–19.
  30. 30. Choy L, Skillington J, Derynck R. Roles of autocrine TGF-beta receptor and Smad signaling in adipocyte differentiation. Journal of Cell Biology. 2000;149(3):667–82.
  31. 31. Caprioli A, Minko K, Drevon C, Eichmann A, Dieterlen-Lievre F, Jaffredo T. Hemangioblast commitment in the avian allantois: cellular and molecular aspects. Developmental Biology. 2001;238(1):64–78.
  32. 32. Choi K, Kennedy M, Kazarov A, Papadimitriou JC, Keller G. A common precursor for hematopoietic and endothelial cells. Development. 1998;125(4):725–32.
  33. 33. Patel-Hett S, D’Amore PA. Signal transduction in vasculogenesis and developmental angiogenesis. International Journal of Developmental Biology. 2011;55(4–5):353–63.
  34. 34. Cox CM, Poole TJ. Angioblast differentiation is influenced by the local environment: FGF-2 induces angioblasts and patterns vessel formation in the quail embryo. Developmental Dynamics: An Official Publication of the American Association of Anatomists. 2000;218(2):371–82.
  35. 35. Dyer MA, Farrington SM, Mohn D, Munday JR, Baron MH. Indian hedgehog activates hematopoiesis and vasculogenesis and can respecify prospective neurectodermal cell fate in the mouse embryo. Development. 2001;128(10):1717–30.
  36. 36. Pepicelli CV, Lewis PM, McMahon AP. Sonic hedgehog regulates branching morphogenesis in the mammalian lung. Current Biology: CB. 1998;8(19):1083–6.
  37. 37. Rowitch DH, B SJ, Lee SM, Flax JD, Snyder EY, McMahon AP. Sonic hedgehog regulates proliferation and inhibits differentiation of CNS precursor cells. Journal of Neuroscience: The Official Journal of the Society for Neuroscience. 1999;19(20):8954–65.
  38. 38. Brown LA, Rodaway AR, Schilling TF, Jowett T, Ingham PW, Patient RK, et al. Insights into early vasculogenesis revealed by expression of the ETS-domain transcription factor Fli-1 in wild-type and mutant zebrafish embryos. Mechanisms of Development. 2000;90(2):237–52.
  39. 39. Byrd N, Becker S, Maye P, Narasimhaiah R, St-Jacques B, Zhang X, et al. Hedgehog is required for murine yolk sac angiogenesis. Development. 2002;129(2):361–72.
  40. 40. Fong GH, Rossant J, Gertsenstein M, Breitman ML. Role of the Flt-1 receptor tyrosine kinase in regulating the assembly of vascular endothelium. Nature. 1995;376(6535):66–70.
  41. 41. Shalaby F, Rossant J, Yamaguchi TP, Gertsenstein M, Wu XF, Breitman ML, et al. Failure of blood-island formation and vasculogenesis in Flk-1-deficient mice. Nature. 1995;376(6535):62–6.
  42. 42. Shalaby F, Ho J, Stanford WL, Fischer KD, Schuh AC, Schwartz L, et al. A requirement for Flk1 in primitive and definitive hematopoiesis and vasculogenesis. Cell. 1997;89(6):981–90.
  43. 43. Ferrara N, Carver-Moore K, Chen H, Dowd M, Lu L, O’Shea KS, et al. Heterozygous embryonic lethality induced by targeted inactivation of the VEGF gene. Nature. 1996;380(6573):439–42.
  44. 44. Kawasaki T, Kitsukawa T, Bekku Y, Matsuda Y, Sanbo M, Yagi T, et al. A requirement for neuropilin-1 in embryonic vessel formation. Development. 1999;126(21):4895–902.
  45. 45. Chen H, Bagri A, Zupicich JA, Zou Y, Stoeckli E, Pleasure SJ, et al. Neuropilin-2 regulates the development of selective cranial and sensory nerves and hippocampal mossy fiber projections. Neuron. 2000;25(1):43–56.
  46. 46. Giger RJ, Cloutier JF, Sahay A, Prinjha RK, Levengood DV, Moore SE, et al. Neuropilin-2 is required in vivo for selective axon guidance responses to secreted semaphorins. Neuron. 2000;25(1):29–41.
  47. 47. Takashima S, Kitakaze M, Asakura M, Asanuma H, Sanada S, Tashiro F, et al. Targeting of both mouse neuropilin-1 and neuropilin-2 genes severely impairs developmental yolk sac and embryonic angiogenesis. Proceedings of the National Academy of Sciences of the United States of America. 2002;99(6):3657–62.
  48. 48. Adams RH, Alitalo K. Molecular regulation of angiogenesis and lymphangiogenesis. Nature Reviews Molecular Cell Biology. 2007;8(6):464–78.
  49. 49. Ribatti D, Nico B, Crivellato E. Morphological and molecular aspects of physiological vascular morphogenesis. Angiogenesis. 2009;12(2):101–11.
  50. 50. Adair TH, Montani JP. Angiogenesis. Integrated Systems Physiology: from Molecule to Function to Disease. San Rafael (CA) 2010.
  51. 51. Rossant J, Howard L. Signaling pathways in vascular development. Annual Review of Cell and Developmental Biology. 2002;18:541–73.
  52. 52. Dickson MC, Martin JS, Cousins FM, Kulkarni AB, Karlsson S, Akhurst RJ. Defective haematopoiesis and vasculogenesis in transforming growth factor-beta 1 knockout mice. Development. 1995;121(6):1845–54.
  53. 53. Akhurst RJ, Lehnert SA, Faissner A, Duffie E. TGF beta in murine morphogenetic processes: the early embryo and cardiogenesis. Development. 1990;108(4):645–56.
  54. 54. Shull MM, Ormsby I, Kier AB, Pawlowski S, Diebold RJ, Yin M, et al. Targeted disruption of the mouse transforming growth factor-beta 1 gene results in multifocal inflammatory disease. Nature. 1992;359(6397):693–9.
  55. 55. Letterio JJ, Geiser AG, Kulkarni AB, Roche NS, Sporn MB, Roberts AB. Maternal rescue of transforming growth factor-beta 1 null mice. Science. 1994;264(5167):1936–8.
  56. 56. Oshima M, Oshima H, Taketo MM. TGF-beta receptor type II deficiency results in defects of yolk sac hematopoiesis and vasculogenesis. Developmental Biology. 1996;179(1):297–302.
  57. 57. Arthur HM, Ure J, Smith AJ, Renforth G, Wilson DI, Torsney E, et al. Endoglin, an ancillary TGFbeta receptor, is required for extraembryonic angiogenesis and plays a key role in heart development. Developmental Biology. 2000;217(1):42–53.
  58. 58. Li DY, Sorensen LK, Brooke BS, Urness LD, Davis EC, Taylor DG, et al. Defective angiogenesis in mice lacking endoglin. Science. 1999;284(5419):1534–7.
  59. 59. Neuzillet C, Tijeras-Raballand A, Cohen R, Cros J, Faivre S, Raymond E, et al. Targeting the TGFbeta pathway for cancer therapy. Pharmacology & Therapeutics [Internet]. 2015;147:22–31 pp. Available from:
  60. 60. Lechleider RJ, Ryan JL, Garrett L, Eng C, Deng C, Wynshaw-Boris A, et al. Targeted mutagenesis of Smad1 reveals an essential role in chorioallantoic fusion. Developmental Biology. 2001;240(1):157–67.
  61. 61. Baird A, Durkin T. Inhibition of endothelial cell proliferation by type beta-transforming growth factor: interactions with acidic and basic fibroblast growth factors. Biochemical and Biophysical Research Communications. 1986;138(1):476–82.
  62. 62. Frater-Schroder M, Muller G, Birchmeier W, Bohlen P. Transforming growth factor-beta inhibits endothelial cell proliferation. Biochemical and Biophysical Research Communications. 1986;137(1):295–302.
  63. 63. Iruela-Arispe ML, Sage EH. Endothelial cells exhibiting angiogenesis in vitro proliferate in response to TGF-beta 1. Journal of Cellular Biochemistry. 1993;52(4):414–30.
  64. 64. Sutton AB, Canfield AE, Schor SL, Grant ME, Schor AM. The response of endothelial cells to TGF beta-1 is dependent upon cell shape, proliferative state and the nature of the substratum. Journal of Cell Science. 1991;99 (Pt 4):777–87.
  65. 65. RayChaudhury A, D’Amore PA. Endothelial cell regulation by transforming growth factor-beta. Journal of Cellular Biochemistry. 1991;47(3):224–9.
  66. 66. Li C, Guo B, Bernabeu C, Kumar S. Angiogenesis in breast cancer: the role of transforming growth factor beta and CD105. Microscopy Research and Technique. 2001;52(4):437–49.
  67. 67. Hofer E, Schweighofer B. Signal transduction induced in endothelial cells by growth factor receptors involved in angiogenesis. Thrombosis and Haemostasis. 2007;97(3):355–63.
  68. 68. Krupinski J, Kumar P, Kumar S, Kaluza J. Increased expression of TGF-beta 1 in brain tissue after ischemic stroke in humans. Stroke; A Journal of Cerebral Circulation. 1996;27(5):852–7.
  69. 69. Dissen GA, Lara HE, Fahrenbach WH, Costa ME, Ojeda SR. Immature rat ovaries become revascularized rapidly after autotransplantation and show a gonadotropin-dependent increase in angiogenic factor gene expression. Endocrinology. 1994;134(3):1146–54.
  70. 70. Pepper MS. Transforming growth factor-beta: vasculogenesis, angiogenesis, and vessel wall integrity. Cytokine & Growth Factor Reviews. 1997;8(1):21–43.
  71. 71. Ferrari G, Pintucci G, Seghezzi G, Hyman K, Galloway AC, Mignatti P. VEGF, a prosurvival factor, acts in concert with TGF-beta1 to induce endothelial cell apoptosis. Proceedings of the National Academy of Sciences of the United States of America. 2006;103(46):17260–5.
  72. 72. Lebrin F, Goumans MJ, Jonker L, Carvalho RL, Valdimarsdottir G, Thorikay M, et al. Endoglin promotes endothelial cell proliferation and TGF-beta/ALK1 signal transduction. EMBO Journal. 2004;23(20):4018–28.
  73. 73. Wang X, Abraham S, McKenzie JA, Jeffs N, Swire M, Tripathi VB, et al. LRG1 promotes angiogenesis by modulating endothelial TGF-beta signalling. Nature. 2013;499(7458):306–11.
  74. 74. McCarty JH, Monahan-Earley RA, Brown LF, Keller M, Gerhardt H, Rubin K, et al. Defective associations between blood vessels and brain parenchyma lead to cerebral hemorrhage in mice lacking alpha v integrins. Molecular and Cellular Biology. 2002;22(21):7667–77.
  75. 75. McCarty JH, Lacy-Hulbert A, Charest A, Bronson RT, Crowley D, Housman D, et al. Selective ablation of alphav integrins in the central nervous system leads to cerebral hemorrhage, seizures, axonal degeneration and premature death. Development. 2005;132(1):165–76.
  76. 76. Proctor JM, Zang K, Wang D, Wang R, Reichardt LF. Vascular development of the brain requires beta8 integrin expression in the neuroepithelium. Journal of Neuroscience: The Official Journal of the Society for Neuroscience. 2005;25(43):9940–8.
  77. 77. Mobley AK, Tchaicha JH, Shin J, Hossain MG, McCarty JH. Beta8 integrin regulates neurogenesis and neurovascular homeostasis in the adult brain. Journal of Cell Science. 2009;122(Pt 11):1842–51.
  78. 78. Aluwihare P, Mu Z, Zhao Z, Yu D, Weinreb PH, Horan GS, et al. Mice that lack activity of alphavbeta6- and alphavbeta8-integrins reproduce the abnormalities of Tgfb1- and Tgfb3-null mice. Journal of Cell Science. 2009;122(Pt 2):227–32.
  79. 79. Hirota S, Clements TP, Tang LK, Morales JE, Lee HS, Oh SP, et al. Neuropilin 1 balances beta8 integrin-activated TGFbeta signaling to control sprouting angiogenesis in the brain. Development. 2015;142(24):4363–73.
  80. 80. Glinka Y, Stoilova S, Mohammed N, Prud’homme GJ. Neuropilin-1 exerts co-receptor function for TGF-beta-1 on the membrane of cancer cells and enhances responses to both latent and active TGF-beta. Carcinogenesis. 2011;32(4):613–21.
  81. 81. Hirota S, Liu Q, Lee HS, Hossain MG, Lacy-Hulbert A, McCarty JH. The astrocyte-expressed integrin alphavbeta8 governs blood vessel sprouting in the developing retina. Development. 2011;138(23):5157–66.
  82. 82. Allinson KR, Lee HS, Fruttiger M, McCarty JH, Arthur HM. Endothelial expression of TGFbeta type II receptor is required to maintain vascular integrity during postnatal development of the central nervous system. PLoS One. 2012;7(6):e39336.
  83. 83. Nguyen HL, Lee YJ, Shin J, Lee E, Park SO, McCarty JH, et al. TGF-beta signaling in endothelial cells, but not neuroepithelial cells, is essential for cerebral vascular development. Laboratory Investigation; A Journal of Technical Methods and Pathology. 2011;91(11):1554–63.
  84. 84. Marchuk DA, Srinivasan S, Squire TL, Zawistowski JS. Vascular morphogenesis: tales of two syndromes. Human Molecular Genetics. 2003;12(Spec No 1):R97–112.
  85. 85. Carvalho RL, Jonker L, Goumans MJ, Larsson J, Bouwman P, Karlsson S, et al. Defective paracrine signalling by TGFbeta in yolk sac vasculature of endoglin mutant mice: a paradigm for hereditary haemorrhagic telangiectasia. Development. 2004;131(24):6237–47.
  86. 86. Su H, Kim H, Pawlikowska L, Kitamura H, Shen F, Cambier S, et al. Reduced expression of integrin alphavbeta8 is associated with brain arteriovenous malformation pathogenesis. American Journal of Pathology. 2010;176(2):1018–27.
  87. 87. Dardiotis E, Siokas V, Zafeiridis T, Paterakis K, Tsivgoulis G, Dardioti M, et al. Integrins AV and B8 gene polymorphisms and risk for intracerebral hemorrhage in Greek and Polish populations. Neuromolecular Medicine. 2016.
  88. 88. Chung AS, Ferrara N. Targeting the tumor microenvironment with SRC kinase inhibition. Clinical Cancer Research: An Official Journal of the American Association for Cancer Research. 2010;16(3):775–7.
  89. 89. Cerami E, Gao J, Dogrusoz U, Gross BE, Sumer SO, Aksoy BA, et al. The cBio cancer genomics portal: an open platform for exploring multidimensional cancer genomics data. Cancer Discovery. 2012;2(5):401–4.
  90. 90. Gao J, Aksoy BA, Dogrusoz U, Dresdner G, Gross B, Sumer SO, et al. Integrative analysis of complex cancer genomics and clinical profiles using the cBioPortal. Science Signaling. 2013;6(269):pl1.
  91. 91. Mazzocca A, Fransvea E, Lavezzari G, Antonaci S, Giannelli G. Inhibition of transforming growth factor beta receptor I kinase blocks hepatocellular carcinoma growth through neo-angiogenesis regulation. Hepatology. 2009;50(4):1140–51.
  92. 92. Akbari A, Amanpour S, Muhammadnejad S, Ghahremani MH, Ghaffari SH, Dehpour AR, et al. Evaluation of antitumor activity of a TGF-beta receptor I inhibitor (SD-208) on human colon adenocarcinoma. Daru: Journal of Faculty of Pharmacy, Tehran University of Medical Sciences. 2014;22:47.
  93. 93. Zhang M, Herion TW, Timke C, Han N, Hauser K, Weber KJ, et al. Trimodal glioblastoma treatment consisting of concurrent radiotherapy, temozolomide, and the novel TGF-beta receptor I kinase inhibitor LY2109761. Neoplasia. 2011;13(6):537–49.
  94. 94. Zhang M, Kleber S, Rohrich M, Timke C, Han N, Tuettenberg J, et al. Blockade of TGF-beta signaling by the TGFbetaR-I kinase inhibitor LY2109761 enhances radiation response and prolongs survival in glioblastoma. Cancer Research. 2011;71(23):7155–67.
  95. 95. Yang XJ, Chen GL, Yu SC, Xu C, Xin YH, Li TT, et al. TGF-beta1 enhances tumor-induced angiogenesis via JNK pathway and macrophage infiltration in an improved zebrafish embryo/xenograft glioma model. International Immunopharmacology. 2013;15(2):191–8.
  96. 96. Deckers MM, van Bezooijen RL, van der Horst G, Hoogendam J, van Der Bent C, Papapoulos SE, et al. Bone morphogenetic proteins stimulate angiogenesis through osteoblast-derived vascular endothelial growth factor A. Endocrinology. 2002;143(4):1545–53.
  97. 97. Ma J, Wang Q, Fei T, Han JD, Chen YG. MCP-1 mediates TGF-beta-induced angiogenesis by stimulating vascular smooth muscle cell migration. Blood. 2007;109(3):987–94.
  98. 98. Hovinga KE, Stalpers LJ, van Bree C, Donker M, Verhoeff JJ, Rodermond HM, et al. Radiation-enhanced vascular endothelial growth factor (VEGF) secretion in glioblastoma multiforme cell lines—a clue to radioresistance? Journal of Neuro-oncology. 2005;74(2):99–103.
  99. 99. Lund EL, Hog A, Olsen MW, Hansen LT, Engelholm SA, Kristjansen PE. Differential regulation of VEGF, HIF1alpha and angiopoietin-1, -2 and -4 by hypoxia and ionizing radiation in human glioblastoma. International Journal of Cancer. 2004;108(6):833–8.
  100. 100. Gupta VK, Jaskowiak NT, Beckett MA, Mauceri HJ, Grunstein J, Johnson RS, et al. Vascular endothelial growth factor enhances endothelial cell survival and tumor radioresistance. Cancer Journal. 2002;8(1):47–54.
  101. 101. Harmey JH, Bouchier-Hayes D. Vascular endothelial growth factor (VEGF), a survival factor for tumour cells: implications for anti-angiogenic therapy. BioEssays: News and Reviews in Molecular, Cellular and Developmental Biology. 2002;24(3):280–3.
  102. 102. Saksela O, Moscatelli D, Rifkin DB. The opposing effects of basic fibroblast growth factor and transforming growth factor beta on the regulation of plasminogen activator activity in capillary endothelial cells. Journal of Cell Biology. 1987;105(2):957–63.
  103. 103. Pollman MJ, Naumovski L, Gibbons GH. Endothelial cell apoptosis in capillary network remodeling. Journal of Cellular Physiology. 1999;178(3):359–70.
  104. 104. Bostrom K, Zebboudj AF, Yao Y, Lin TS, Torres A. Matrix GLA protein stimulates VEGF expression through increased transforming growth factor-beta1 activity in endothelial cells. Journal of Biological Chemistry. 2004;279(51):52904–13.
  105. 105. Hamerlik P, Lathia JD, Rasmussen R, Wu Q, Bartkova J, Lee M, et al. Autocrine VEGF-VEGFR2-Neuropilin-1 signaling promotes glioma stem-like cell viability and tumor growth. Journal of Experimental Medicine. 2012;209(3):507–20.
  106. 106. Cheng L, Huang Z, Zhou W, Wu Q, Donnola S, Liu JK, et al. Glioblastoma stem cells generate vascular pericytes to support vessel function and tumor growth. Cell. 2013;153(1):139–52.
  107. 107. Bruna A, Darken RS, Rojo F, Ocana A, Penuelas S, Arias A, et al. High TGFbeta-Smad activity confers poor prognosis in glioma patients and promotes cell proliferation depending on the methylation of the PDGF-B gene. Cancer Cell. 2007;11(2):147–60.
  108. 108. Roy LO, Poirier MB, Fortin D. Transforming growth factor-beta and its implication in the malignancy of gliomas. Targeted Oncology. 2015;10(1):1–14.
  109. 109. Louis DN. Molecular pathology of malignant gliomas. Annual Review of Pathology. 2006;1:97–117.
  110. 110. Doerr M, Morrison J, Bergeron L, Coomber BL, Viloria-Petit A. Differential effect of hypoxia on early endothelial-mesenchymal transition response to transforming growth beta isoforms 1 and 2. Microvascular Research. 2016;108:48–63.
  111. 111. Platten M, Wick W, Wild-Bode C, Aulwurm S, Dichgans J, Weller M. Transforming growth factors beta(1) (TGF-beta(1)) and TGF-beta(2) promote glioma cell migration via Up-regulation of alpha(V)beta(3) integrin expression. Biochemical and Biophysical Research Communications. 2000;268(2):607–11.
  112. 112. Brooks PC, Stromblad S, Sanders LC, von Schalscha TL, Aimes RT, Stetler-Stevenson WG, et al. Localization of matrix metalloproteinase MMP-2 to the surface of invasive cells by interaction with integrin alpha v beta 3. Cell. 1996;85(5):683–93.
  113. 113. Tchaicha JH, Mobley AK, Hossain MG, Aldape KD, McCarty JH. A mosaic mouse model of astrocytoma identifies alphavbeta8 integrin as a negative regulator of tumor angiogenesis. Oncogene. 2010;29(31):4460–72.
  114. 114. Tchaicha JH, Reyes SB, Shin J, Hossain MG, Lang FF, McCarty JH. Glioblastoma angiogenesis and tumor cell invasiveness are differentially regulated by beta8 integrin. Cancer Research. 2011;71(20):6371–81.

Written By

Paola A. Guerrero and Joseph H. McCarty

Submitted: 09 June 2016 Reviewed: 19 October 2016 Published: 05 April 2017