• Loading metrics

A computational analysis of in vivo VEGFR activation by multiple co-expressed ligands

A computational analysis of in vivo VEGFR activation by multiple co-expressed ligands

  • Lindsay E. Clegg, 
  • Feilim Mac Gabhann


The splice isoforms of vascular endothelial growth A (VEGF) each have different affinities for the extracellular matrix (ECM) and the coreceptor NRP1, which leads to distinct vascular phenotypes in model systems expressing only a single VEGF isoform. ECM-immobilized VEGF can bind to and activate VEGF receptor 2 (VEGFR2) directly, with a different pattern of site-specific phosphorylation than diffusible VEGF. To date, the way in which ECM binding alters the distribution of isoforms of VEGF and of the related placental growth factor (PlGF) in the body and resulting angiogenic signaling is not well-understood. Here, we extend our previous validated cell-level computational model of VEGFR2 ligation, intracellular trafficking, and site-specific phosphorylation, which captured differences in signaling by soluble and immobilized VEGF, to a multi-scale whole-body framework. This computational systems pharmacology model captures the ability of the ECM to regulate isoform-specific growth factor distribution distinctly for VEGF and PlGF, and to buffer free VEGF and PlGF levels in tissue. We show that binding of immobilized growth factor to VEGF receptors, both on endothelial cells and soluble VEGFR1, is likely important to signaling in vivo. Additionally, our model predicts that VEGF isoform-specific properties lead to distinct profiles of VEGFR1 and VEGFR2 binding and VEGFR2 site-specific phosphorylation in vivo, mediated by Neuropilin-1. These predicted signaling changes mirror those observed in murine systems expressing single VEGF isoforms. Simulations predict that, contrary to the ‘ligand-shifting hypothesis,’ VEGF and PlGF do not compete for receptor binding at physiological concentrations, though PlGF is predicted to slightly increase VEGFR2 phosphorylation when over-expressed by 10-fold. These results are critical to design of appropriate therapeutic strategies to control VEGF availability and signaling in regenerative medicine applications.

Author summary

Angiogenesis, the growth of new blood vessels from the existing vasculature, is critical for maintenance of health and response to injury. In ischemic disease, this process is impaired, but therapies targeting a key family of proteins, the vascular endothelial growth factors (VEGF), have failed to translate clinically. This suggests a need for deeper understanding of the complex regulation underlying angiogenic signaling. Here, we translate a previously developed and validated model of VEGF family signaling into a human, whole-body framework. The different splice isoforms of VEGF and the related PlGF proteins have different affinities for the extracellular matrix (ECM) and the co-receptor Neuropilin-1. Using our model, we examine the effect of these different binding properties on the distribution of each isoform in tissue, and subsequent receptor signaling. The model predicts isoform-specific receptor activation that is consistent with observed vascular phenotypes in mice expressing a single VEGF isoform; non-ECM-binding isoforms lead to signaling that promotes cell proliferation, while strong ECM-binding promotes migratory signaling and increased vessel branching. This understanding is critical for design of biomaterials that manipulate VEGF-ECM binding to control growth factor delivery, and for understanding of splicing-induced changes in VEGF family signaling in different tissues and in disease.


Angiogenesis, the growth of new capillaries from the existing vasculature, is critical for maintenance of health and response to injury, as well as being a component of many diseases. However, regulation of angiogenesis is highly complex [1], and not fully understood. This complexity is a key reason for the lack of approved, effective therapies to promote angiogenesis for tissue engineering applications [24], for wound healing [5], or for ischemic diseases such as peripheral artery disease (PAD) [6], despite much research and multiple clinical trials [7]. Thus, a more complete, mechanistic understanding of the regulation of angiogenesis is crucial to designing more effective pro-angiogenic therapies.

Key to angiogenesis is the vascular endothelial growth factor (VEGF) family, including VEGF-A, VEGF-B, VEGF-C, VEGF-D, and placental growth factor (PlGF). VEGF-A (hereafter referred to as VEGF), considered the primary pro-angiogenesis VEGF ligand, has multiple splice isoforms, the most prevalent in humans being VEGF121, VEGF165, and VEGF189. Constitutive dimers of these splice isoforms bind to VEGF-receptor 1 (VEGFR1) and VEGF-receptor 2 (VEGFR2). Upon ligand binding, VEGF receptors dimerize, transphosphorylate, and initiate downstream signaling [810].

The longer two prevalent human VEGF isoforms (VEGF165 and VEGF189) contain heparin-binding domains, allowing for binding to heparan sulfate proteoglycans (HSPGs) in the extracellular matrix (ECM). These isoforms also have binding sites for the coreceptor Neuropilin-1 (NRP1), which regulates VEGF affinity for VEGFR2 and influences VEGFR2 trafficking, though the less-common heparin-binding VEGF145 does not bind to NRP1 [11, 12]. These isoform-specific properties have physiological significance; upon secretion into the extracellular space, VEGF121, which does not bind to the ECM or to NRP1, forms shallow gradients and diffuses away from the source of production, while VEGF189, which binds strongly to the ECM and also binds NRP1, forms steep interstitial gradients and remains close to the site of production [13].

In addition, mice and tumors expressing single VEGF isoforms have distinct phenotypes. Expression of only VEGF121 leads to formation of high diameter vessels with low branching density, while expression of only VEGF189 results in highly branched networks of very thin vessels. By contrast, expression of VEGF165 alone results in a phenotypically normal vasculature, with balanced branching and diameters [1417]. In addition to regulating VEGF distribution, it has recently been shown that the immobilization of VEGF to ECM proteins or to a surface alters the site-specific phosphorylation profile of VEGFR2 in vitro. While phosphorylation of tyrosine Y1175, which leads to ERK1/2 activation and cell proliferation, is similar whether VEGF is immobilized or presented in solution, phosphorylation of Y1214, which leads to phosphorylation of p38 and cell migration, increases when VEGF is immobilized [18, 19]. This shift in signaling, which parallels the phenotypes seen with single VEGF isoform expression, can be explained by reduced internalization of VEGFR2 bound to immobilized VEGF, altering the exposure of VEGFR2 to specific phosphatases, as we recently demonstrated via a computational model of VEGFR2 signaling in vitro [20].

PlGF is not as well-studied as VEGF-A, in part because it is not required for normal murine development and homeostasis [21], and in part because PlGF binds only to VEGFR1, and not to VEGFR2, which is often considered to be the primary signaling receptor [22]. Like VEGF, PlGF has multiple splice isoforms, namely PlGF1 and PlGF2, with only the longer isoform (PlGF2) binding to ECM proteins strongly, and also to NRP1 [23, 24]. Despite being dispensable for murine development, PlGF expression is different in humans than mice [25], and increasing evidence implicates PlGF in disease [26]. Structural similarity also allows VEGF and PlGF to form heterodimers when produced in the same cells [27, 28]. There is high inter-study and intra-study variability in measurements of PlGF in human plasma and serum [2941], many of which are from pregnant women, but levels of PlGF in healthy subjects are generally higher than those of VEGF-A (in 6 of 8 studies reviewed in [42] where both VEGF and PlGF in plasma or serum were measured [2936]), and lower than those of soluble VEGFR1 (in 4 of 5 studies reviewed in [42] measuring both PlGF and sR1 in human plasma or serum [32, 3437]).

VEGFR1 is also understudied compared to VEGFR2. VEGFR1 kinase activity appears to be weaker than that of VEGFR2, but VEGFR1 binds to VEGF more strongly than VEGFR2 [10]. While VEGFR1 kinase activity is not required for normal murine development [43], it appears to be important in the adult vasculature [4446]. Like the VEGF ligands, VEGF receptors have alternative splice forms. Specifically, soluble VEGFR1 (sR1) is a naturally-occurring splice isoform lacking the transmembrane and intracellular domains but maintaining the ligand-, NRP1-, and HSPG-binding sites of VEGFR1. sR1 is secreted by endothelial cells into the extracellular space [47, 48]. There, sR1 can bind to the ECM [49] and/or bind to VEGF and PlGF, potentially preventing these growth factors from binding to cell surface receptors. Additionally, sR1 may heterodimerize with cell surface receptor monomers, forming non-signaling complexes [50]. While VEGF binding to VEGFR1 is thought by some to be anti-angiogenic, PlGF-induced VEGFR1 activation is generally considered to be pro-angiogenic [2]; the tyrosine phosphorylation patterns on VEGFR1 induced by VEGF and PlGF are different [44], and PlGF-VEGFR1 signaling is pro-angiogenic in zebrafish [51]. It has been hypothesized, based on in vitro data and overexpression studies, that PlGF and VEGFB binding to VEGFR1 induces pro-angiogenic effects by occupying VEGFR1, shifting VEGF from VEGFR1 to VEGFR2 [44, 5254].

Though the contributions of VEGF, PlGF, growth factor immobilization, sR1, NRP1, VEGFR1, and VEGFR2 to VEGF-mediated signaling have all been studied in vitro (and to a limited extent in vivo), the combined regulation of these cues in the context of the human body is not well-understood. Compared to in vitro studies, physiological ligand concentrations are very low, many different growth factors are constantly being produced, consumed, and transported throughout the body, and the time-scales of interest are far longer [55]. Computational models provide a key tool to study the combined effects of many forms of regulation within a single framework, and to scale between model systems and human patients.


The primary objectives of this study were: (1) to predict the distribution of VEGF and PlGF within the body, (2) to understand the effect of VEGF and PlGF on the balance of VEGFR1 and VEGFR2 ligation and VEGFR2 phosphorylation, (3) to quantify the effect of matrix-bound VEGF & PlGF binding to endothelial and soluble receptors on VEGFR signaling, and (4) to study the impact of changes in VEGF & PlGF isoform expression on absolute and relative VEGFR1 & VEGFR2 activation and site-specific phosphorylation of VEGFR2, as a result of isoform-specific matrix- and NRP1-binding properties, all within the context of a healthy human body.

The computational systems pharmacology model developed in this study is based on previously-developed computational models of VEGF distribution and receptor binding in vivo. These models have included VEGF165, VEGF121, VEGFR1, VEGFR2, soluble VEGFR1 (sR1), NRP1, and sites in the interstitial matrix to which some growth factors and sR1 can bind [5658]. The distribution of these proteins and their complexes has been examined in tissues of therapeutic interest (healthy or PAD calf [58], or tumor [59, 60]), the blood, and non-diseased tissue (main body mass) [56, 57], in humans or mice [61, 62], incorporating transport between these compartments via vascular permeability and lymphatic drainage of tissues, and clearance of proteins from the plasma. By including multiple tissue compartments, we can compare quantities in a tissue of interest to those in the bulk of body tissue.

In the present study, we greatly expand upon previous models to further capture the complexity of VEGF distribution and VEGF receptor activation in the body. For the first time, we include two isoforms of placental growth factor (PlGF1 & PlGF2), and the VEGF isoform VEGF189. Additionally, we account for binding of matrix-immobilized ligands in the endothelial basement membrane (EBM) to cell-surface receptors (VEGFR1 & VEGFR2), binding of immobilized ligands throughout the interstitial space to soluble sR1, and the ability of sR1, when sequestered in the interstitial matrix, to bind some VEGF isoforms. To capture these effects, we simulate receptor trafficking and VEGFR2 tyrosine site-specific phosphorylation following ligand binding or unbinding explicitly, implementing the reactions in a previously-developed in vitro computational model that captures differences in VEGFR2 phosphorylation following stimulation with soluble or matrix-bound VEGF165 [20]. Finally, we leverage recent measurements to update endothelial cell surface receptor densities [63].


Compartmental model formulation

To capture the pharmacokinetics of VEGF, PlGF, and sR1 distribution in the human body, we divide the body into three compartments: a healthy calf muscle (gastrocnemius + soleus muscles), blood, and the main body mass (the rest of the tissues), approximated with the properties of skeletal muscle (Fig 1A). Transport between compartments occurs via bi-directional vascular permeability and lymphatic drainage of tissues (into the blood), while growth factors and sR1 are cleared from the blood (via the liver and kidneys), using rates previously determined (S10 Table). Each tissue compartment includes physiological proportions of interstitial space, extracellular matrix (ECM), endothelium, other parenchymal cells, and basement membranes for both the endothelium and parenchyma (endothelial- EBM, and parenchymal- PBM).

Fig 1. Schematics of molecular detail and structure of multi-scale computational model.

(A) Whole-body compartmental model structure and mass flow. VEGF and PlGF are secreted from parenchymal cells, and sR1 is secreted by endothelial cells into the tissue interstitial space. Ligands and sR1 can then bind to EC receptors (leading to internalization and degradation), and can be transported between the tissue and blood via bi-directional vascular permeability or lymphatic draining of tissues into the circulation. Soluble species in the blood can be directly cleared from the blood. (B) Molecular interactions in tissue interstitial space between VEGF121, VEGF165, VEGF189, PlGF1, PlGF2, NRP1, sR1, and extracellular HSPGs/GAGs (M). It is assumed that, similar to NRP1-VEGFR1 complexes, VEGF121 and PlGF1 can bind to sR1-M. ECM-bound VEGF165, VEGF189, and PlGF2 can also bind to sR1. (C) Trafficking processes simulated in endothelial cells. (D) Site-specific phosphorylation and dephosphorylation of VEGFR2. (E) Abluminal (tissue-side) endothelial cell-surface molecular interactions between VEGF121, VEGF165, VEGF189, PlGF1, PlGF2, VEGFR1, VEGFR2, NRP1, sR1, and extracellular HSPGs/GAGs in the endothelial basement membrane (EBM).

Within each tissue, we incorporate molecularly-detailed pharmacodynamics, including secretion into the interstitial space of VEGF and PlGF by parenchymal cells and sR1 by endothelial cells. In the interstitium, these diffusible proteins can then bind to heparan sulfate proteoglycans (HSPGs) in the ECM and basement membranes (see Fig 1B, S11 Table), bind to receptors on endothelial cells (ECs), or be removed from the compartment via physiological transport processes (Fig 1A). VEGF and PlGF isoforms have different affinities for matrix sites and for the coreceptor NRP1, which are included (Table 1), to account for isoform-specific ligand distribution and receptor activation. On the surface of and within endothelial cells, we simulate binding of sR1 to NRP1, binding of PlGF to VEGFR1 and/or NRP1, and binding of VEGF to VEGFR1, VEGFR2, and/or NRP1, based on the binding properties of each protein (summarized in Tables 13 and Fig 1E).

Endothelial cell surface receptors are continually produced, internalized, recycled, and degraded, with trafficking rates that depend on ligation status and complex formation with NRP1 (Fig 1C). We include detailed VEGFR2 trafficking based on a previous in vitro computational model (S8 Table). Surface receptor production rates were tuned to match experimental measurements of cell surface receptor levels in human umbilical vein endothelial cells (Table 4). We also explicitly include phosphorylation and site-specific dephosphorylation of VEGFR2 (Fig 1D), which is dependent on receptor trafficking, with higher net activation at Y1214 than Y1175 on the cell surface, and higher Y1175 phosphorylation in early (Rab4/5) endosomes (S9 Table), as a result of differential dephosphorylation of Y1175 and Y1214 on the cell surface and in early endosomes [20]. This allows us to study phosphorylation explicitly, instead of using receptor occupancy as a surrogate, and to look at relative activation of downstream signaling pathways leading to proliferation (pY1175 via ERK1/2) and migration (pY1214 via p38).

Due to the spatially-averaged nature of this model, gradients and heterogeneity in growth factor, soluble receptor, and cell surface receptor patterning are neglected. Instead, we examine the tissue-averaged behavior within the context of the human body. We neglect secretion of sR1 directly into the bloodstream, receptors present on the luminal side of ECs, and degradation of growth factors by proteases. All parameters are based on or fit to experimental data, either newly here or previously for other computational models. By building on previous modeling efforts, we have built more molecular detail into our models, while adding only a modest number of new parameters (indicated in bold in Tables 14 and S7 Table).

To simulate the time-course of each molecular species in each tissue and the blood, this model includes 635 nonlinear ordinary differential equations that are solved simultaneously. The model equations can be found in S1 Equations. The full set of differential equations was solved in Fortran using the Livermore Solver for Ordinary Differential Equations with Automatic method switching for stiff and nonstiff problems (LSODA), on a laptop PC, with a relative error tolerance of 10−6.

Model parameterization


The geometric parameterization is taken, without modification, from a previous 3-compartment model of a healthy 70 kg human [57], and is detailed in S7 Table. Briefly, histological cross-sections of human gastrocnemius muscle and vastus lateralis muscle were used to parameterize the “calf muscle” and “main body mass” compartments, respectively. These cross-sections and other measurements were used to estimate the relative fractions of muscle volume occupied by myocytes, capillaries (separated into vascular space and endothelium), and interstitial space. Estimates of endothelial and myocyte basement membrane thickness, cell surface areas and volumes, and the volume fractions of ECM protein and fluid in interstitial space were also used to parameterize the tissue compartments. For full details, see [57]. The blood is taken to be 5L, with 60% of that volume being plasma.

Binding and coupling kinetics.

In this model, we include five growth factor ligands (L), each with different receptor-binding, matrix-binding, and NRP1-binding properties (Fig 1B and 1E). Our goal is to understand how these isoform-specific properties lead to differential ligation and activation of VEGFR1 and VEGFR2. We assume all ligands and receptors are pre-dimerized, neglecting the formation of ligand or receptor heterodimers, and assume the same binding properties for sR1 as endothelial VEGFR1 [70]. NRP1 can bind directly to VEGFR1 (and we assume sR1) [71], while VEGF is required to bridge NRP1 and VEGFR2. While VEGF binds to both VEGFR1 and VEGFR2, PlGF binds to only VEGFR1. The shorter PlGF1 does not bind to NRP1 or to the matrix (M), but we assume that PlGF1, like VEGF121, does bind to VEGFR1 and NRP1 simultaneously. VEGF121 does not bind to the matrix, and its ability to bind NRP1 [72] alone is neglected, as it has previously been shown to have very little effect on VEGFR signaling in vivo [57]. For both PlGF and VEGF, the longer isoforms (VEGF165, VEGF189, and PlGF2) bind to the matrix, PlGF2 more strongly than VEGF165 [66]. These longer isoforms also bind NRP1, but not NRP1-VEGFR1 complexes (though this remains unproven for PlGF2). Reflecting our previous in vitro computational model, we account for binding of matrix-bound ligands to VEGFR2 (previously demonstrated [18, 19]) and VEGFR1 (assumed to occur). We assume that endothelial basement membrane-bound growth factor within 25nm of the cell surface is accessible to cell surface receptors, based on the length of the extracellular domain of the related RTKs ErbB2 and ErbB3 (11.3–16.4nm) [7375], and assuming some flexibility in cell position and shape. We calculated the resulting fraction of EBM accessible to cell surface receptors (S7 Table), and scaled the corresponding reaction on-rates (Table 2, see S1 Equations). Similarly, we allow matrix-immobilized VEGF165, VEGF189, or PlGF2 to bind to sR1, creating matrix-ligand-sR1 (M-L-sR1) complexes, which cannot bind cell surface receptors, and are therefore effectively sequestered. As VEGFR1 can bind to NRP1 without ligand, and the NRP1- and heparin-binding domains of VEGFR1 overlap, we also examine the impact of allowing matrix-bound sR1 to bind VEGF121 and PlGF1 in the interstitial space, allowing these non-matrix-binding ligands to be sequestered. In all cases, in the absence of evidence to the contrary, we assume that matrix-immobilization does not affect the affinity of any interactions.

The binding and unbinding rates for VEGF and PlGF to VEGFR1, VEGFR2, and sR1 are kept the same as in previous models [45, 57], as summarized in Tables 13 (new parameters in bold). Though we have not previously included PlGF in a compartment model, PlGF binding to VEGFR1 has been modeled in vitro [45], and the parameter values are matched to this study. The affinity of PlGF2 for NRP1 is based on experimental measurements of PlGF2 binding to the NRP1 extracellular domain [65]. Slightly different affinities are used for VEGF binding to matrix sites and to NRP1 than in previous compartment models, in order to use measurements from a single source for both VEGF165 and VEGF189 (NRP1-binding) [64], or for VEGF and PlGF (matrix-binding) [66]. Since VEGF189 is known to bind the ECM more strongly than VEGF165, but an affinity is not available, we assume 10x stronger binding, similar to the difference in VEGF165 and VEGF189 affinity for NRP1 [64]. As in previous models [57], lacking a measured affinity for sR1 binding to matrix, we assume a value similar to that for VEGF, as both interactions occur via heparin-binding domains.

Receptor trafficking and VEGFR2 phosphorylation.

We added receptor trafficking and VEGFR2 phosphorylation to the model, in order to track site-specific phosphorylation of VEGFR2 explicitly, rather than simply receptor occupancy. This is more accurate, as in vitro VEGFR2 phosphorylation decreases faster than can be accounted for by ligand depletion or receptor degradation [20]. We implemented these reactions as previously described in an in vitro model [20] for VEGFR2, accounting for ligand-induced changes in internalization, recycling, and degradation, as well as preferential recycling of VEGFR2 complexes containing NRP1 via a Rab11-dependent pathway. The trafficking rate constants are given in S8 Table. Though VEGFR1 trafficking is known to be distinct from that of VEGFR2 [76, 77], we lack sufficient data to build or validate a model of VEGFR1 trafficking. As such, a structure for VEGFR1 trafficking was incorporated for future use, but results are presented only for cell surface VEGFR1.

Site-specific phosphorylation of VEGFR2 on three tyrosine sites is included: Y951, Y1175, and Y1214. We approximate phosphorylation and dephosphorylation as first order processes, and assume that these processes occurred independently on each tyrosine. The phosphorylation rate is assumed to be zero for unoccupied VEGFR2, and fast (1 s-1) for ligated VEGFR2. The dephosphorylation rates do not depend directly on the VEGF isoform, but vary by tyrosine site and subcellular location (S9 Table), as previously fit and validated [20] using experimental observations of increased pY1214 following stimulation with immobilized VEGF compared to free VEGF in solution [18], and enabling site-specific phosphorylation patterns to depend on the mixture of matrix- binding and non-matrix-binding isoforms available to VEGFR2. Given limited data available for phosphorylation of Y951 upon which to fit the model, this analysis focuses on VEGFR2 activation on Y1175 and Y1214.


Inter-compartmental transport parameters are taken from a previous model [57] (see S10 Table). Vascular permeability was estimated based on the Stokes-Einstein radii for each protein. Here, we assume the same permeability for PlGF as VEGF, as they have similar molecular weights and are structurally related. Lymphatic drainage transports proteins from tissue compartments to the blood in a tissue-mass-dependent and a protein-size-independent fashion. We use the estimated lymphatic flow rates for a supine, awake 70 kg human [57].

Protein expression levels.

We assume the same densities of interstitial matrix sites available to bind VEGF, PlGF, and sR1 in the ECM and basement membranes as used in previous models [57] (see S11 Table). Briefly, ECM binding-site density is based on measured FGF binding sites [78, 79], while basement membrane binding site densities are estimated based on Engelbreth-Holm-Swarm sarcomas in diabetic mice [80]. Endothelial cell surface VEGFR1, VEGFR2, and NRP1 target levels were chosen to match median experimental (FACS) measurements in human umbilical vein endothelial cells [63, 67], which represented our best information to date on receptor levels in humans; these values are summarized in Table 4. Total receptor levels are not directly controlled, but remain within a reasonable range. The VEGF and PlGF secretion rates by myocytes and endothelial secretion of sR1 into the interstitial space were adjusted to match experimentally measured plasma protein levels (Table 4). Plasma levels are used as targets because no interstitial measurements of sR1 or PlGF levels are available, and plasma VEGF levels are better characterized than tissue interstitial levels. Target levels of plasma VEGF and sR1 are unchanged from previous models [57], and a plasma PlGF target concentration of 10pM was selected. The secretion of different VEGF isoforms and PlGF isoforms are maintained at fixed ratios, based on experimental measurements in mice (VEGF) and humans (PlGF) [68, 69]. Production rates for VEGFR1, VEGFR2, and NRP1 were adjusted independently in the calf muscle and the main body mass to meet target values in each tissue while also meeting plasma ligand targets. As VEGF, PlGF, and sR1 secretion are fit only to plasma measurements, we assume the same secretion rates per cell in both tissue compartments.


Ligand secretion and receptor production rates for baseline typical healthy human

The ligand secretion and receptor production rates necessary to hit baseline (healthy) targets had to be fit simultaneously, due to the highly non-linear nature of the system. At our baseline steady-state, the VEGF production rate is 0.2830 molecules/myonuclear domain/s, the PlGF production rate is 0.0146 molecules/myonuclear domain/s, and the sR1 production rate is 0.0893 molecules/EC/s (see Table 4). The VEGF and sR1 production rates here are higher than previous estimates. This is unsurprising, given the changes in receptor levels, trafficking, and growth factor isoforms. Surprisingly, the PlGF production rate is lower than that for VEGF, despite a higher target plasma level (see Flux Analysis section for the mechanism by which this occurs).

To illustrate the nonlinearity of our model, we perturbed each ligand secretion and receptor production rate slightly (2%), and examined changes in plasma ligand and tissue receptor levels. As shown in Fig 2A, plasma VEGF and tissue VEGFR2 are highly sensitive to changes in either VEGF secretion or VEGFR2 production in the main body mass, with changes of 11–25% per percent change in input. As VEGF levels increase, more VEGFR2 becomes occupied, internalized, and degraded, reducing VEGFR2 levels and decreasing VEGF consumption (Fig 2B and S1 Fig). Similarly, as VEGFR2 production increases, more VEGF is bound to VEGFR2, internalized, and degraded, reducing VEGF levels and thus increasing EC surface VEGFR2. This super-sensitivity was not present in previous models, where surface VEGFR2 levels were fixed (see S1 Fig). This new, emergent result suggests that, lacking upregulation of VEGFR2 in response to VEGF, VEGFR2 levels would be highly sensitive to even small fluctuations in local VEGF concentration (Fig 2), highlighting the importance of dynamic adjustments to ligand and receptor expression in vivo. In the calf muscle, perturbing VEGFR2 production has a large impact on EC surface VEGFR2, but little effect on plasma VEGF, due to the smaller size of the compartment. Changes in receptor production in one tissue compartment have little effect on receptor levels in the other tissue compartment.

Fig 2. Nonlinearity of ligand & sR1 secretion and EC receptor production rates in the model.

(A) One at a time, each baseline ligand secretion or receptor production rate (inputs- listed across the top), was increased by 2%, then decreased by 2%. For each perturbation, the change in plasma ligand and EC surface receptor levels (outputs- listed on the left) in in both the main body mass (“Body”) and calf muscle (“Calf”) were obtained. The average change in output from baseline levels was calculated, and divided by the change in input (+/-2%) to give the relative change in output per % change in input. (B) Schematic of positive feedback in VEGF gene and protein levels in the model. An increase in VEGF expression increases local VEGF protein, increasing VEGF binding to VEGFR2, and subsequent internalization and degradation. This decreases total VEGFR2 protein levels, leading to reduced VEGF-VEGFR2 complex formation, which reduces net endothelial consumption of VEGF protein. To accommodate, in the model, VEGFR2 expression was increased until target baseline levels were achieved for all ligands and receptors. A similar positive feedback loop exists for changes in VEGFR2 expression.

In this model, we assume the same rates for ligand production in both the healthy calf muscle and the main body mass. As such, perturbing the VEGF secretion rate (in both compartments) alters the receptor levels in both tissues (Fig 2). Due to differences in the geometric parameterizations of the calf and other tissues (S7 Table), using the same ligand secretion rates results in different interstitial VEGF, sR1, and PlGF levels (Fig 3D). We focus primarily on quantities measured in the “Main Body Mass” compartment, which, due to its larger size, represents the primary determinant of plasma VEGF, sR1, and PlGF levels.

Fig 3. Pharmacokinetics of VEGF, PlGF, and sR1 at steady-state.

(A) Predicted free and sR1-bound ligands, and free and ligand-bound sR1 in plasma. (B) Predicted VEGF, PlGF, and sR1 distribution in healthy tissue in “Main Body Mass” compartment, shown in pM of tissue. (C) Extracellular (not bound to or inside ECs) VEGF, PlGF, and sR1 in “Main Body Mass” compartment, in pM of tissue. (D) Steady-state net flow profiles for VEGF, PlGF, sR1, and sR1-ligand complexes between the calf muscle, blood, and main body mass. All VEGF isoforms are aggregated, as are both PlGF isoforms. Green arrows represent production, red arrows EC consumption, black arrows bi-directional vascular permeability, gray arrows lymphatic drainage, and pink arrows with red outlines direct clearance from blood. The white arrows show the net association or dissociation of VEGF-sR1 and PlGF-sR1 complexes in each compartment. Displayed concentrations are free ligand, sR1, or complex in interstitial fluid or plasma. The numbers under each compartment are the respective compartment volumes. Flows are given in pmoles/day. (E) Comparison of VEGF and PlGF isoform distribution with relative isoform production rates demonstrates locations and complexes where each isoform is under- or over-represented relative to the fraction of total VEGF or PlGF production. (F) Matrix site occupancy in the EBM, ECM, and PBM.

Pharmacokinetics: Where are VEGF, PlGF, and sR1 in the body?

After establishing the secretion and production rates required to achieve basal targets, we next examined the steady-state distribution of VEGF, PlGF, and sR1.

Plasma: Differential isoform representation compared to relative expression levels.

In the plasma, free VEGF protein is predicted to be 84% VEGF165, 7% VEGF121, and 9% VEGF189; thus VEGF189 (the strongest ECM-binding isoform) is underrepresented compared to the production fractions of 77%, 8%, and 15%, respectively (Fig 3A and 3E). Conversely, the ECM-binding PlGF2 isoform is overrepresented in plasma (98% of free plasma PlGF), compared to its production (85% of PlGF production), reflecting its overrepresentation in the tissue extracellular space (see Fig 3). In agreement with previous models, 77% of plasma VEGF and 39% of PlGF are bound to sR1. A total of 10% of plasma sR1 is bound to ligand, with 44% of this bound to VEGF and 56% bound to PlGF, suggesting that PlGF interacts with sR1 to a comparable extent as VEGF.

Tissue (Main Body Mass): ECM-binding drives distinct VEGF & PlGF isoform distribution.

The model predicts that the total and relative levels of matrix-bound and free growth factor are dictated by ECM binding properties (Fig 3C). While the model predicts that the majority of VEGF121, VEGF165, and PlGF1 are bound to endothelial cells (96%, 62%, and 58%, respectively- see Fig 3B) in the main body mass, large portions of the heparin-binding isoforms, VEGF165, VEGF189, and PlGF2, are bound to the ECM and basement membranes (36%, 74%, and 99.6% of total in tissue, respectively), alone or in complex with sR1 (Fig 3B). Most of the immobilized growth factor is in the ECM and parenchymal BM (Fig 3C), inaccessible to EC receptors, but available for proteolytic release. Total extracellular (non-EC-bound) VEGF is 48% VEGF165, only 2% VEGF121, and 50% VEGF189, while extracellular PlGF is 99.97% PlGF2 (Fig 3E). As these percentages suggest, most extracellular heparin-binding growth factor is matrix bound (alone or in complex with sR1): 96% of VEGF165, 99.6% of VEGF189, and 99.7% of PlGF2. However, 93% of VEGF121 and 80% of PlGF1 are also sequestered (via immobilized sR1) in our simulations. The total amount of sequestered VEGF121 and PlGF1 is small (Fig 3C), but still significant compared to the corresponding free growth factor concentrations in solution. Indeed, only 7.8% of tissue PlGF1 and <1% of every other isoform is predicted to be “free” in solution. This is consistent with previous results [57] in suggesting that, unlike cell culture experiments, ligand-receptor binding is limited by ligand availability in the body. The model predicts that 90% of sR1 in tissue is matrix-bound (Fig 3B), while only 0.45% is free (bound to neither matrix nor ligand), and 0.32% bound to ligand alone, implicating the ECM in regulation of sR1 distribution as well.

While a large fraction of growth factor is immobilized, predicted matrix site occupancy is low (2.4%- see Fig 3F). This is higher than in previous models, as a result of the inclusion of PlGF and immobilized complexes containing both growth factor and sR1. In the endothelial BM, most (93%) occupied sites contain PlGF; 16% contain sR1, and 2.3% VEGF. While only 1.1% of occupied EBM sites include ligand bound to cell surface receptors, the large number of binding sites in the endothelial BM makes even this small fraction physiologically relevant (see Fig 4).

Fig 4. Pharmacodynamics of ligand binding to VEGFR1 and VEGFR2.

(A) Total soluble growth factor (in available interstitial fluid) and immobilized growth factor (in innermost 25nm of EBM) accessible to ECs. Growth factor bound to EC receptors is not included in this plot. (B) Break-down of EC surface-bound ligand, by isoform. Note the difference in quantities of total ligated VEGFR2, VEGFR1, and NRP1 (panel C). (C) Occupancy of VEGFR2, VEGFR1, and NRP1 on ECs, broken down by ligand and NRP1-binding. VEGFR2 occupancy is shown on the cell surface, in early signaling endosomes (Rab4/5), and in recycling endosomes (Rab11), while VEGFR1 and NRP1 are shown only on the cell surface. Quantities are given in pM of total tissue in the “Main Body Mass” compartment. (D) VEGFR2, VEGFR1, and NRP1 ligation on ECs, excluding receptor not bound to ligand. Complexes not listed in the legend are present at levels too low to be seen in the figure. (E) Break-down of percentage of EC surface VEGFR1 and VEGFR2 ligation comprised by each isoform, compared to the relative production of each isoform. Production fractions are calculated separately for VEGF and PlGF, while for receptor binding the combined distribution is shown.

Flux analysis: Differential transport of VEGF & PlGF.

By calculating the net transport, consumption, and clearance of each protein or complex (Fig 3D), we can examine the contributions of each dynamic process to the steady-state distribution. At steady-state, the model predicts a concentration of 11pM VEGF in the available interstitial fluid of the main body mass, similar to previous models. The levels in the calf muscle are higher (20pM), due to a higher myocyte volume fraction and resulting higher production per unit tissue volume. While other quantities also varied between the two compartments, all trends and net flux directions were the same. In agreement with previous model predictions, free sR1 levels are higher in plasma than in tissue, while PlGF levels, like VEGF levels, are higher in tissue. These concentration differences lead to predicted transendothelial intravasation (net transfer from tissue to blood) of VEGF and PlGF, while free sR1 is predicted to extravasate (net transfer from blood to tissue). The fraction of sR1 bound to ligand is similar in plasma and tissue interstitial fluid (42% in the main body mass, 51% in calf muscle), with substantial contributions by both VEGF and PlGF. The large majority of VEGF and sR1 produced are consumed locally by endothelial cells (99% of VEGF and 98% of sR1 in the “Main Body Mass”), accounting for the high sensitivity of interstitial VEGF to VEGFR2 production (see Fig 2). Conversely, the model predicts that only 25% of PlGF is consumed by ECs, due to much lower total binding to EC receptors than VEGF. This accounts for the low PlGF production rate required to match target plasma levels, and suggests that PlGF may be primarily cleared via transendothelial transport and lymphatic drainage into plasma, followed by clearance from the blood, or by cell types not included in this model (e.g. monocytes & macrophages).

Pharmacodynamics: What controls VEGFR1 and VEGFR2 activation?

Having examined the distribution of VEGF, PlGF, and sR1, we next zoomed in to examine the effect of these proteins and their distributions on the binding and activation of endothelial VEGFR1 and VEGFR2 within healthy tissue.

Growth factors levels are limiting for in vivo EC receptor activation.

At steady state, cell surface ligation of VEGFR2 is predicted to be close to an order of magnitude higher than cell surface ligation of VEGFR1 (Fig 4D), due in part to higher levels of EC surface VEGFR2 (5800 VEGFR2/cell vs. 1800 VEGFR1/cell). As a result, the majority of EC consumption of VEGF occurs via VEGFR2, explaining why VEGF levels are more sensitive to changes in production of VEGFR2 than VEGFR1 (Fig 2). Overall, the model predicts low cell surface receptor occupancies of 3.4% for VEGFR1 and 8.7% for VEGFR2 (4.5% VEGFR1 and 14% VEGFR2 in calf muscle), and somewhat higher but still low total (surface + endosomal) VEGFR2 occupancy (20%), suggesting that ligands do not compete for receptor binding (Fig 4C). This prediction is conservative; model VEGF levels are in fact higher than estimates of free interstitial VEGF via microdialysis, and plasma target levels for VEGF and PlGF assume that no sR1-bound ligand was detected. While sR1 is known to interfere with VEGF ELISA measurements, likely at least a portion of this bound VEGF is in fact detected, thus placing our calibrated model at the top of the possible VEGF range.

NRP1- & ECM-binding drive VEGF & PlGF isoform binding to VEGFR1 and VEGFR2.

The majority of non-ligand-bound VEGFR1 is predicted to be in complex with NRP1 (99.1%). NRP1 remains mostly free (95.3%) (Fig 4C), with some binding to sR1 and PlGF2 to form non-signaling complexes (Fig 4D). The isoform-specific NRP1 binding properties of VEGF and PlGF make NRP1 a strong regulator of ligand-binding to VEGFR1 and VEGFR2. The model predicts that VEGF165 and VEGF189, which bind to VEGFR2 and NRP1 simultaneously, bind almost exclusively to VEGFR2 (Fig 4D). Conversely, VEGF121, which binds to NRP1-VEGFR1 complexes, comprise 70% of ligand bound to VEGFR1 (Fig 4D), while PlGF makes up only 29% of the ligand bound to VEGFR1 at steady-state (Fig 4E). This result explains the lower predicted occupancy of VEGFR1 than VEGFR2; VEGF121 and PlGF1, the only ligands to bind VEGFR1 and NRP1 simultaneously, represent a small fraction of total ligand (Fig 4A). The dominance of VEGF121 binding to endothelial VEGFR1 is in contrast to the relatively even binding of VEGF and PlGF to sR1 (Fig 2), and occurs because most tissue PlGF is PlGF2, which cannot bind to NRP1-VEGFR1 complexes on endothelial cells.

While all soluble growth factors are accessible to EC receptors in this model (assuming a well mixed compartment, i.e. nonlimiting fast diffusion), cell surface receptors are only allowed to bind to immobilized ligands in the innermost 25nm of endothelial BM. A substantial fraction of both soluble and endothelial BM-bound growth factor is bound to sR1, and thus inaccessible to EC receptors (Fig 4A). Of the remaining growth factor, the model predicts that the amount of available free growth factor exceeds the amount of available immobilized growth factor for all VEGF isoforms, but not for PlGF2 (Fig 4A) However, within the 25nm space adjacent to endothelial cells, the concentration of available immobilized growth factor far exceeds the predicted concentration of free growth factor for all matrix-binding isoforms (S2A Fig).

Of the 0.03% of basement membrane sites bound to ligand-cell surface receptor complexes, 23% are immobilized PlGF2 bound to VEGFR1, 20% are VEGF165-R2 complexes, and 56% are VEGF189-R2 complexes. While more of these complexes are bound to VEGFR2, VEGFR1 has a higher fraction of ligand-receptor complexes bound to immobilized ligands (18% versus 6.9%- see Fig 4D). This is due the lower total number of ligand-VEGFR1 complexes, combined with higher tissue levels and stronger matrix binding by PlGF2 compared to VEGF. If we assumed all endothelial BM-bound growth factors were accessible to receptors (as opposed to the closest 25nm), 50% of ligated VEGFR1 would be bound to immobilized PlGF, and 17% of ligated VEGFR2 would be bound to immobilized VEGF165 or VEGF189.

NRP1 regulates isoform-specific trafficking and phosphorylation of VEGFR2.

In addition to guiding receptor ligation, NRP1 also regulates VEGFR2 trafficking [11], speeding up recycling of ligated VEGFR2. This leads to predicted accumulation of VEGF121-VEGFR2 complexes in early signaling (Rab4/5) endosomes, while VEGF165-VEGFR2 and VEGF189-VEGFR2 are recycled back to the cell surface, leading to a more even distribution between the cell surface and early endosomes (Fig 4D). As such, changes in relative levels of VEGF isoforms are predicted to alter not only the tissue distribution of ligand and the balance of VEGFR1 and VEGFR2 activation, but also the subcellular localization of VEGFR2.

We previously showed that changes in site-specific phosphorylation of VEGFR2 as a function of VEGF165 immobilization to a surface or in a gel could be explained by prolonged retention of immobilized VEGF-VEGFR2 complexes at the cell surface [20], increasing net phosphorylation on Y1214 and promoting pro-migratory signaling. Here, we examined whether this translated to VEGF isoform-specific trends in site-specific phosphorylation of VEGFR2 in a physiological context. Indeed, we see that the faster dephosphorylation of tyrosine Y1175 than Y1214 on the cell surface, and vice versa in early (Rab4/5) signaling endosomes (Fig 5B), leads to different relative levels of VEGFR2 activation on Y1175 and Y1214 as a function of the bound ligand; the heparin-binding VEGF isoforms (VEGF165 and VEGF189) lead to higher net activation on Y1214, while VEGF121 shifts relative activation towards Y1175 (Fig 5C).

Fig 5. VEGF isoform-specific trafficking and site-specific phosphorylation of VEGFR2 in vivo.

(A) VEGF isoform-specific NRP1-binding properties result in isoform-specific trafficking of VEGFR2. (B) Subcellular location-specific dephosphorylation rates for Y1175 and Y1214 (S9 Table) lead to preferential activation of tyrosine 1214 on the EC surface, compared to signaling in endosomes. (C) Isoform-specific trafficking and location-specific dephosphorylation combine to result in isoform-specific trends in relative activation of VEGFR2 on tyrosine 1175 and tyrosine 1214. (D) Total VEGFR2 phosphorylation, on at least one tyrosine (pR2) and specifically on Y1175 or Y1214, across all subcellular locations. (E-F) Distribution of pY1175 (E) and pY1214 (F), by VEGF isoform and location.

Complex, coordinated regulation of VEGFR1 and VEGFR2 signaling

It is clear that the different proteins—ligands, soluble receptors, and co-receptors—regulating VEGFR1 and VEGFR2 activation do not act in isolation. Changes to any single feature affect the total multi-factor system in a way that is difficult to predict without the use of a computational model. Here, we perturb several interactions that are of interest therapeutically, and/or are included in this model for the first time.

PlGF does not displace VEGF from VEGFR1 to increase VEGFR2 signaling in vivo.

To test the ‘ligand-shifting hypothesis,’ i.e. that PlGF induces pro-angiogenic effects in vivo by shifting VEGF binding from VEGFR1 to VEGFR2, we altered the amount of PlGF production in tissue, and quantified the resulting changes in cell surface VEGFR1 ligation and total VEGFR2 phosphorylation. To control for changes in cell surface VEGFR1 and total VEGFR2, we normalized these quantities by the relevant receptor population. We found, across a wide range of PlGF production (from zero to 10x baseline levels), that despite large changes in free PlGF levels in tissue (Fig 6A), only modest changes in VEGFR2 ligation and phosphorylation (pR2/R2) were observed (Fig 6B). Conversely, VEGFR1 ligation changes much more (varying from 69% to 389% of baseline VEGFR1 ligation) with PlGF levels. The shift in VEGFR1 ligation is almost entirely due to PlGF; VEGFR1 ligation by VEGF remains approximately constant (Fig 6C). These results suggest that, while at supraphysiologic concentrations (>10x baseline), PlGF may increase VEGFR2 phosphorylation, PlGF and VEGF do not compete for VEGFR1 binding in physiological conditions. This is consistent with the low predicted receptor occupancies, and our previous in vitro simulations [45, 46], but is demonstrated here for the first time for in vivo scenarios.

Fig 6. Complex regulation of VEGF family signaling by PlGF, EBM binding sites, and sR1.

(A-C) Changes in free ligand levels in tissue interstitial fluid (A), EC surface VEGFR1 ligation and VEGFR2 phosphorylation (B), and the breakdown of VEGF and PlGF bound to EC surface VEGFR1 (C), in response to varying PlGF production. Quantities shown are normalized to baseline cases. (D-F) Effect of endothelial basement membrane (EBM) binding site density on EBM site occupancy (D), fraction of occupied EBM sites bound to different ligands and receptors (E), and VEGFR1 and VEGFR2 ligation by immobilized VEGF or PlGF (F). (G-I) Total activation of VEGFR1 and VEGFR2 (G), and break-down of relative ligation by each VEGF and PlGF isoform (H-I) with varying sR1 production.

VEGFR1 ligation is more sensitive than VEGFR2 ligation to matrix site density.

While the model predicts that less than 20% of ligated endothelial cell surface receptors are bound to immobilized ligand, the total number of accessible binding site in the endothelial BM is not well-characterized, nor is the fraction of the basement membrane accessible to EC surface receptors. Thus, we examined whether, if growth factor binding sites in the endothelial BM are present at higher or lower density than estimated, a difference in cell surface receptor ligation would be predicted. As we increased the density of accessible sites from baseline levels by factors of 10 and 100, the fraction of cell surface ligated VEGFR2 bound to immobilized VEGF increased, reaching 48% (compared to 6.9% at baseline) with a 100-fold increase in binding site density (Fig 6F). Interestingly, the fraction of ligated cell surface VEGFR1 bound to immobilized ligand (largely PlGF2) increases more quickly with endothelial BM site density, reaching 76% with 10x, and 97% with 100x, compared to 17% at baseline. These results suggest that immobilized ligand-receptor complexes may be important in vivo (Fig 6F).

sR1 alters the magnitude of receptor activation more than the profile of receptor-bound ligands.

Since plasma sR1 levels are known to change in disease, we examined the extent to which sR1 can act in an anti-angiogenic manner to modulate endothelial VEGFR1 and VEGFR2 activation. To do this, we simulated knockdown or overexpression of sR1. As expected, free tissue VEGF and PlGF and ligation of both VEGFR1 and VEGFR2 increases (1.9- and 1.5-fold increases in ligation, respectively) with complete sR1 knockout (Fig 6G). Similarly, overexpression of sR1 reduces EC receptor ligation substantially, but does not completely block binding. Interestingly, the effect is more pronounced on VEGFR1 than VEGFR2, shifting the overall balance of signaling by VEGFR1 vs. VEGFR2 (Fig 6G). We examined whether sR1 perturbation would affect the profiles of ligands bound to VEGFR1 and VEGFR2 (Fig 6H and 6I). We observed little change in the ligand bound to VEGFR2. Changes to VEGFR1 ligation are larger, with relative PlGF binding increasing and relative VEGF121 binding decreasing with increasing sR1 production.

Immobilized ligand binding to sR1 regulates ligand distribution, binding to EC receptors regulates EC signaling.

Next, we examined the relative contribution of immobilized complexes containing sR1 versus EC receptors to our observed results. We compared four cases: (1) the baseline case where 3-element complexes of matrix, VEGF or PlGF, and either sR1 or EC VEGFR1 and VEGFR2 were allowed to form, (2) a case excluding all such reactions (No MLR), (3) a case allowing these reactions on sR1 but not EC receptors (sR1 Only), and (4) a case allowing these reactions on EC receptors but not sR1 (Cell Only). For each case, we re-fit the secretion and production rates to hit our plasma and cell surface receptor targets (S12 Table). We found that sR1 binding to immobilized ligands has a large impact on the amounts of free and total growth factor in tissue (Fig 7). Conversely, EC receptor binding to immobilized ligand increases receptor ligation and phosphorylation. Combined, these effects produce the observed differences between the baseline and No MLR cases.

Fig 7. Immobilized ligand binding to sR1 alters tissue distribution, while immobilized ligand binding to EC receptors alters activation state.

Panels show percent change from baseline. Thus, the smallest bars indicate little impact of the removed reactions on a given output, while large bars indicate large change when the reactions are removed. Cell Only: Immobilized ligand allowed to bind to EC receptors, but not sR1. Binding of ligand to immobilized sR1 is also not allowed. sR1 Only: Immobilized ligand allowed to bind to sR1, and ligand to immobilized sR1, but binding of immobilized ligand to EC receptors is not included. No MLR: No matrix-ligand-receptor or matrix-ligand-sR1 complexes are allowed to form. Top: Changes in fit ligand secretion and receptor production rates to match plasma ligand and sR1 targets and tissue EC surface receptor targets. Middle: Distribution of free, total, and matrix-bound VEGF and PlGF. Bottom: EC receptor activation.

Model predictions of signaling in human body with expression of only single VEGF isoforms are consistent with observed murine vascular phenotypes

The most convincing evidence to date of differential signaling by VEGF isoforms is the distinct vascular phenotypes of mice or human tumors (implanted in mice) expressing only single isoforms of VEGF, with VEGF121-only tissues producing high diameter, sparsely branched networks, VEGF165-only tissue a relatively normal phenotype, and VEGF189-only tissues networks of thin, highly branched vessels. Endothelial cells isolated from these single isoform-expressing mice also display distinct signaling and behavior in cell culture [81]. It is assumed that similar regulation occurs in humans. To better understand VEGF isoform-specific signaling in the context of the human, as well as to qualitatively validate our model, we simulated expression of a single VEGF isoform in the human body. While no significant changes in VEGFR1 or VEGFR2 mRNA were observed in the muscle of mice expressing only VEGF120 [82] (equivalent to human VEGF121), we re-fit our model for each case, in order to maintain target ligand and receptor levels (S13 Table). The need for these changes in receptor production and ligand secretion rates may be a result of differences between humans and mice, or underlying compensation mechanisms and physiological changes in the engineered mice [82] not included in this model. Consistent with observations in mice, ligand distribution and VEGFR2 activation are more similar to wild type (baseline) in the VEGF165-only than the VEGF121-only or VEGF189-only cases (Fig 8A and 8B). Similar to the baseline case (Fig 5), where all three isoforms are expressed, with single VEGF isoform expression the ratio of migratory to proliferative signaling downstream of VEGFR2 (pY1214/pY1175) is predicted to increase with isoform length, paralleling the observed phenotypes (Fig 8C). The model’s ability to capture this trend provides qualitative validation of our isoform-specific signaling predictions in vivo. Interestingly, the model also predicts other changes, in free VEGF levels in tissue interstitium (Fig 8A) and in relative activation of VEGFR1 and VEGFR2 (Fig 8B and 8D, S1 File).

Fig 8. Predicted signaling changes in the human body with expression of single VEGF isoforms mirror experimentally observed murine phenotypes.

(A) Levels of free VEGF, PlGF, and sR1 in tissue interstitial fluid, normalized to baseline, when all VEGF production is VEGF121, VEGF165, or VEGF189. (B) Endothelial cell surface ligation of VEGFR1 and phosphorylation of VEGFR2. Changes in pR2 and ligated VEGFR2 were very similar. (C) Ratio of total VEGFR2 phosphorylation on tyrosine Y1214 to phosphorylation of tyrosine Y1175. (D) Percent of ligated EC surface VEGFR1 and VEGFR2 bound to EBM-immobilized ligand.


We constructed this computational systems pharmacology model to probe the complexity of VEGF family distribution and signaling in the body, for the first time accounting for the impact of PlGF and of receptor binding by basement membrane-immobilized ligands. In demonstrating the contribution of multiple specific mechanisms to regulation of VEGF family signaling, this model explores the sometimes non-intuitive effects these complex interactions have on VEGFR1 and VEGFR2 activation. This model is based on previously-developed compartment models, leveraging the same structure and geometric parameterization. Despite this commonality, adding to and improving the molecular-level detail resulted in changes to some model predictions, as well as the ability to predict VEGFR2 signaling in more detail than was previously possible (see Fig 9A).

Fig 9. Summary of key model predictions.

(A) Overview of key predictions. (B) Due to differences in NRP1- and ECM-binding, VEGF isoform-VEGFR2 complexes are trafficked differently, leading to distinct downstream signaling, cellular behavior, and vascular network architecture. (C) Summary of predicted ligand binding to VEGFR1 and VEGFR2. All ligands in the respective boxes can bind to VEGFR1 or VEGFR2. The size of the ligands represents the predicted contribution to receptor binding in vivo. The model suggests that, for each receptor, a subset of the ligands dominate.

Model provides novel insight into PlGF transport and potential for VEGFR1-dependent PlGF signaling

Our model predicts that, based on their binding properties and in vivo concentrations, PlGF and VEGF have distinct distributions within the body. PlGF2, binding to the ECM more strongly than VEGF, is bound to interstitial matrix sites at very high levels (~1 nM in tissue: soluble + ECM-bound + EC-bound predicted, Fig 3C), forming a large reservoir available for proteolytic release. Despite high tissue PlGF levels, our simulations predict that only about 30% of ligated EC surface VEGFR1 is bound to PlGF. As a result, while most VEGF removal from tissue is predicted to occur via binding to endothelial receptors, only 25% of PlGF was predicted to bind to and be subsequently degraded by endothelial cells. PlGF also binds VEGFR1 on other cells, e.g. monocytes and macrophages, that are implicated in arteriogenesis [26, 83]. We found that removing PlGF or increasing PlGF secretion has only a modest effect on predicted VEGFR2 phosphorylation, while substantially altering VEGFR1 activation (Fig 6A). This result suggests that observed physiological PlGF-dependent pro-angiogenic effects are likely mediated directly by VEGFR1, either on ECs or other cells, and not via changes in VEGFR2 signaling, contrary to the ‘ligand-shifting hypothesis’. This result implicates VEGFR1 in the impaired angiogenic responses to ischemia, wound healing, and cancer [21] observed in mice lacking PlGF. It also implicates VEGFR1 in diseases where PlGF levels are known to change or to be predictive of prognosis, e.g. pre-eclampsia [42] and breast cancer [84]. The pro-angiogenic effects of PlGF likely also rely on its ability to up-regulate other growth factors, including VEGF, FGF2, and PDGF [85, 86].

This result is not inconsistent with recent work by the Alitalo group showing that therapeutic over-expression of VEGFB (which like PlGF binds only VEGFR1) in mice improves metabolic health even following endothelial Flt1 gene deletion, and inhibits doxorubicin-induced cardiotoxicity [54, 87]. Competition between ligands is concentration-dependent, and in these studies, VEGFB protein levels were elevated 20-fold or more in serum, heart, liver, and white adipose tissue. Our model predicts that competition is not a driver of PlGF signaling in physiological conditions, but does not preclude the existence of competition following supraphysiologic therapy. Indeed, at 10-fold PlGF over-expression, outside of the concentration range likely to be observed in untreated healthy or diseased tissue [42], the model does begin to predict an effect on VEGFR2 signaling.

Growth factor immobilization and binding to soluble VEGFR1 predicted to be important for VEGF family signaling in vivo

Both the ECM and sR1 regulate tissue levels of free interstitial VEGF and PlGF, the amount of growth factor available to bind ECs, and the steady-state distribution of ligand throughout the body (Fig 3). The model predicts that sR1 modulates the magnitude of EC receptor ligation, potentially also altering the balance of signaling via VEGFR1 vs. VEGFR2 (Fig 6G). This is of therapeutic interest because ratios of VEGF or PlGF to sR1 levels in plasma are increasingly of interest as a biomarker (e.g. in pre-eclampsia) [70], and sR1 levels increase in diabetic mice following hindlimb ischemia [88]. Including binding of immobilized ligands to sR1, and binding of immobilized sR1 to VEGF121 and PlGF1, increases total extracellular VEGF and PlGF stored in tissue (Fig 7). While there is not yet evidence to prove the existence of such complexes, the heparin- and ligand-binding sites on sR1 are distinct, as are the heparin- and receptor-binding domains on VEGF and PlGF, and therefore these complexes are likely.

Unlike matrix-ligand-sR1 complexes, VEGF immobilized to both surfaces and ECM proteins has been shown to bind and activate VEGFR2 in vitro, preferentially increasing VEGFR2 activation of tyrosine Y1214, upstream of p38 phosphorylation and migratory cell behavior, demonstrating an important role for physical immobilization of VEGF in signal regulation in vitro [18, 19, 89]. However, whether VEGFR2 ligation by immobilized VEGF would occur to any notable extent in vivo, and what the physiological impact on EC receptor signaling would be, have been unknown. Here, we saw that including these reactions increased EC receptor ligation and altered VEGFR2 signaling (Fig 7). While the number of available sites in the EBM is not well-established, our model suggests that these M-L-R complexes may make up a small but significant portion of ligated EC receptors (Fig 4D). To improve our estimates of the extent of EC receptor ligand by EBM-bound growth factor, it is necessary to obtain better estimates of heparin-binding sites in basement membranes. Interestingly, the fraction of ligated VEGFR1 bound to immobilized ligand was predicted to be higher than that for VEGFR2, owing largely to the strong M-PlGF2 affinity (Fig 6F). To date, the impact of VEGFR1 ligation by immobilized ligand has not been studied. However, as these are largely PlGF2-VEGFR1 complexes (Fig 6F), EBM binding site density may shift relative ligation of VEGFR1 by VEGF versus PlGF, which is known to alter VEGFR1-mediated signaling [44]. Spatial patterning of receptor ligation by soluble and immobilized ligand is also likely to be important, but cannot be examined with this model. Additionally, the potential roles for HSPGs and NRP1 expressed on other cells engaging with VEGFR2 in trans [90, 91] are of interest for future study.

Model predicts VEGF isoform-specific activation of VEGFR1 and VEGFR2

We were interested in differences in signaling between VEGF isoforms upon binding to VEGFR1 and VEGFR2. Explicitly simulating VEGFR2 trafficking and site-specific phosphorylation, placed in the context of physiological geometry and transport processes, allowed us to predict isoform-specific VEGFR2 signaling in vivo (Fig 5). Immobilization in the matrix alters VEGF distribution and the resulting signaling, while NRP1 alters VEGF-receptor binding and trafficking. By including these isoform-specific properties, the model predicts that VEGF121 induces a shift in VEGFR2 distribution towards early signaling endosomes, decreasing the signaling ratio pY1214/pY1175, and shifting the net cellular signaling towards proliferation. Conversely, a larger portion of VEGFR2 bound to VEGF189 was localized on the EC surface at steady-state, increasing pY1214/pY1175, and shifting the balance towards pro-migratory signaling (Fig 5C). This isoform-specific patterning in VEGFR2 signaling was seen in both the baseline case (Fig 5C), with all three VEGF isoforms present, and in cases where only single isoforms of VEGF were expressed (Fig 8C). This is key validation, as our simulated signaling predictions in humans match the observed vascular phenotypes in mice or tumors expressing single VEGF isoforms (Fig 9B). Interestingly, in the single isoform cases, change in relative activation of VEGFR1 and VEGFR2 were also predicted (Fig 8B), which may contribute to these phenotypes [92, 93].

This is in line with another interesting model prediction; while all VEGF isoforms can bind to both VEGFR1 and VEGFR2, physiologically it appears that VEGF165 and VEGF189 bind almost exclusively to VEGFR2, while VEGF121 comprises a large portion of the ligand on VEGFR1, and also binds VEGFR2 to an extent (Fig 4D). This segregation of ligands suggests that, while ligand levels are limiting for receptor binding, VEGFR1 and VEGFR2 don’t directly compete for VEGF in vivo, instead binding to largely distinct subsets of ligands dictated primarily by isoform-specific NRP1-binding properties (Fig 9C). The relative levels of VEGF isoforms are not yet extensively-characterized, but they are known to vary by tissue and to change in disease [69, 82, 94, 95]. As such, this model can be used to understand splicing-induced tissue- and disease-specific changes in VEGF receptor signaling.

Considerations for interpretation of model predictions

Our model is built upon experimental data and a validated model of VEGFR2 signaling in vitro, and provides new insight into distribution of and signaling by VEGF and PlGF isoforms in vivo. However, when interpreting the results, it is important to acknowledge mismatch between model predictions and experimental measurements, which may result from limitations of our modeling approach, uncertainly in interpretation of experimental measures, and/or missing understanding of underlying biological mechanism. Similar to previous models, our predicted interstitial VEGF concentrations when fitting the model to measured plasma VEGF levels are higher than those measured in tissues using microdialysis. This discrepancy could be due to: difficulty in obtaining accurate measurements for high molecular weight proteins using microdialysis; production of VEGF by blood sources (e.g. PBMCs, platelets) or specific organs (e.g. highly fenestrated tissue), reducing the requisite VEGF production by skeletal muscle; or degradation of VEGF by tissue-resident proteases and/or other cell types expressing VEGF receptors (modeled in [96, 97]). Inclusion of proteases in the model would reduce immobilized growth factor stores at steady state. Additionally, as in previous models, the predicted fraction of plasma sR1 bound to ligand was higher than the experimentally-measured fraction. There are other soluble receptors that may be important to consider and are not included here. There may also be limitations with the experimental method that make these in vivo measurements inaccurate. To quantify the importance of some difficult-to-measure parameters, as well as reactions included in this model for the first time (some of which have not been explicitly demonstrated experimentally), we analyzed the sensitivity of many new or poorly characterized parameters (see S3 Fig and S1 File).

In order to achieve simulation at the whole body scale, compartment models neglect spatial effects, instead predicting only average values for tissue. The interstitial space of the tissue, the cell surface of endothelial cells and the cell surface of myocytes are still independent entities in this case and each is treated as well-mixed. Detailed study of gradients in interstitial space and along cell surfaces, which are difficult to measure in vivo but are likely key to angiogenic signaling, requires development of detailed 2- and 3-dimensional models of tissue and experimental set-ups, calibrated to match predicted average concentrations from compartment models [98101] such as the one presented here. Much work remains to fully understand the role of spatial gradients of VEGF distribution and receptor activation in health, disease, and response to therapy.


This model integrates detailed regulation of VEGF and PlGF distribution and binding to EC VEGFR1 and VEGFR2 by sR1, the ECM, and NRP1 into a multi-scale pharmacokinetic/pharmacodynamic (PK/PD) framework. The resulting model predicts that all of these features interact, and contribute to regulation of tissue-level VEGF family signaling. While many model predictions are difficult to validate in vivo, the mechanisms included were first modeled using detailed in vitro measurements, and validated in many cases on the cellular level, before being put in a physiological context using an existing PK/PD framework. By progressively adding complexity, we can study the impact of each contribution, and compare simulation results to quantities that are measurable and to observable phenotypes, such as the vascular morphologies in mice expressing single isoforms of VEGF. By the same turn, this model provides a window into details of growth factor distribution and signaling that are essentially impossible to measure (especially on the protein level), though in many cases implicated in disease-related impairment in angiogenic response, or targeted by potential therapies. The lack of approved pro-angiogenic therapies to date makes it clear that a better understanding of the molecular mechanisms driving disease is critical to identify more effective drug targets, optimize drug properties (e.g. affinity), and avoid off-target effects leading to toxicity and drug failure [55]. This work can be extended to disease applications with changes in VEGF splicing, and to compare results in humans versus mice, to aid in translation of therapeutics targeting the VEGF system and to further validate the model against data obtained in mice.

Supporting information

S1 Fig. Super-sensitivity of steady-state VEGF and VEGFR2 levels, compared to previous model set-up.

These panels expands upon the results shown in Fig 2 of the main manuscript. (A) In previous models, surface VEGFR2 levels were fixed (same internalization rate for free and VEGF-bound VEGFR2, no recycling), so increasing VEGF levels would lead to more VEGF-VEGFR2 binding and subsequent degradation of VEGF, keeping the net change in VEGF levels relatively small. (B) In this model, trafficking rates are different for free and ligand-bound VEGFR2, so endothelial cell surface VEGFR2 levels are not constant when VEGF levels change. If VEGF levels increase, more VEGFR2 becomes occupied, internalized, and degraded, reducing steady-state VEGFR2 levels and decreasing VEGF consumption via VEGFR2 (purple). Similarly, if VEGFR2 production increases, more VEGF is bound to VEGFR2, internalized, and degraded, reducing steady-state VEGF levels and as a result further increasing surface VEGFR2 (green).


S2 Fig. Additional pharmacokinetic/pharmacodynamic predictions of the model.

(A) This panel, which shows “local” concentrations of growth factor accessible to endothelial cell receptors, is related to Fig 4A of the main manuscript. EBM-bound growth factor concentrations are calculated using the EBM volume, while free levels are calculated using the total available interstitial space. (B) This panel expands upon the results shown in Fig 5 of the main manuscript. For each isoform, total phosphorylated VEGFR2 (pR2) bound to the given ligand is divided by total VEGFR2 bound to the respective ligand.


S3 Fig. Sensitivity of transport parameters and new or unconfirmed reactions.

(A) Sensitivity of ligand distribution and receptor activation to changes in, from left to right: NRP1 production rate (sN1), vascular permeability (kp), lymphatic drainage rate (kL), and rate of clearance from the blood (kCL). All tissue quantities are taken from the “Main Body Mass” compartment. Values shown are the average magnitude of change in a given quantity when the specified parameter is increased or decreased by a factor of 10 (baseline = 0). Note the different scale on the NRP1 production rate than on the other panels. (B) Changes to ligand distribution and receptor activation when kon for different reactions is set to zero, prohibiting the selected reactions from occurring. Values shown are fold change from baseline (baseline = 1). Examined reactions are, from left to right: binding of sR1 to EC NRP1 (with or without ligand), binding of ligand to sR1-N1 complexes, binding of PlGF1 to NRP1-VEGFR1 and NRP1-sR1 complexes, formation of immobilized ligand-VEGFR1 and immobilized ligand-sR1 complexes (in any form), binding of VEGF121 or PlGF1 to immobilized sR1, binding of free sR1 to matrix proteins (no ligand), binding of immobilized ligands to sR1 (only), and binding of matrix proteins to VEGF165, VEGF189, or PlGF2 bound to sR1. All tissue quantities taken from “Main Body Mass” compartment. Note the different scale on the sR1-N1 and P1-(N1-R1) panels than on the other panels.


S1 Table. Binding/Unbinding reactions: KD in the main body mass.


S2 Table. Binding/Unbinding reactions: KD in healthy calf muscle.


S3 Table. Binding/Unbinding reactions: KD in plasma.


S4 Table. Binding/Unbinding reactions: kon in the main body mass.


S5 Table. Binding/Unbinding reactions: kon in healthy calf muscle.


S6 Table. Binding/Unbinding reactions: kon in plasma.


S12 Table. Production and secretion rates for “MLR” cases (Fig 7).


S13 Table. Production and secretion rates for single VEGF isoform cases (Fig 8).


Author Contributions

  1. Conceptualization: LEC FMG.
  2. Formal analysis: LEC.
  3. Funding acquisition: FMG.
  4. Investigation: LEC.
  5. Methodology: LEC FMG.
  6. Resources: LEC FMG.
  7. Software: LEC.
  8. Validation: LEC FMG.
  9. Visualization: LEC FMG.
  10. Writing – original draft: LEC.
  11. Writing – review & editing: LEC FMG.


  1. 1. Clegg LE, Mac Gabhann F. Systems biology of the microvasculature. Integrative Biology. 2015.
  2. 2. Mac Gabhann F, Qutub AA, Annex BH, Popel AS. Systems biology of pro-angiogenic therapies targeting the VEGF system. Wiley Interdisciplinary Reviews-Systems Biology and Medicine. 2010;2(6):694–707. pmid:20890966
  3. 3. Lovett M, Lee K, Edwards A, Kaplan DL. Vascularization Strategies for Tissue Engineering. Tissue Engineering Part B-Reviews. 2009;15(3):353–70. pmid:19496677
  4. 4. Auger FA, Gibot L, Lacroix D. The Pivotal Role of Vascularization in Tissue Engineering. Annual Review of Biomedical Engineering, Vol 15. 2013;15:177–200.
  5. 5. Briquez PS, Hubbell JA, Martino MM. Extracellular Matrix-Inspired Growth Factor Delivery Systems for Skin Wound Healing. Advances in Wound Care. 2015.
  6. 6. Grochot-Przeczek A, Dulak J, Jozkowicz A. Therapeutic angiogenesis for revascularization in peripheral artery disease. Gene. 2013;525(2):220–8. pmid:23566831
  7. 7. Briquez PS, Clegg LE, Martino MM, Gabhann FM, Hubbell JA. Design principles for therapeutic angiogenic materials. Nature Reviews Materials. 2016;1:15006.
  8. 8. Mac Gabhann F, Popel AS. Systems biology of vascular endothelial growth factors. Microcirculation (New York, NY: 1994). 2008;15(8):715–38.
  9. 9. Koch S, Tugues S, Li X, Gualandi L, Claesson-Welsh L. Signal transduction by vascular endothelial growth factor receptors. Biochemical Journal. 2011;437:169–83. pmid:21711246
  10. 10. Koch S, Claesson-Welsh L. Signal Transduction by Vascular Endothelial Growth Factor Receptors. Cold Spring Harbor Perspectives in Medicine. 2012;2(7).
  11. 11. Ballmer-Hofer K, Andersson AE, Ratcliffe LE, Berger P. Neuropilin-1 promotes VEGFR-2 trafficking through Rab11 vesicles thereby specifying signal output. Blood. 2011;118(3).
  12. 12. Gluzman-Poltorak Z, Cohen T, Herzog Y, Neufeld G. Neuropilin-2 and neuropilin-1 are receptors for the 165-amino acid form of vascular endothelial growth factor (VEGF) and of placenta growth factor-2, but only neuropilin-2 functions as a receptor for the 145-amino acid form of VEGF. Journal of Biological Chemistry. 2000;275(24):18040–5. pmid:10748121
  13. 13. Vempati P, Popel AS, Mac Gabhann F. Extracellular regulation of VEGF: Isoforms, proteolysis, and vascular patterning. Cytokine & Growth Factor Reviews. 2014;25(1):1–19.
  14. 14. Park JE, Keller GA, Ferrara N. Vascular endothelial growth factor (VEGF) isoforms- Differential deposition into the subepithelial extracellular-matrix and bioactivity of extracellular matrix-bound VEGF. Molecular Biology of the Cell. 1993;4(12):1317–26. pmid:8167412
  15. 15. Ruhrberg C, Gerhardt H, Golding M, Watson R, Ioannidou S, Fujisawa H, et al. Spatially restricted patterning cues provided by heparin-binding VEGF-A control blood vessel branching morphogenesis. Genes & Development. 2002;16(20):2684–98.
  16. 16. Grunstein J, Masbad JJ, Hickey R, Giordano F, Johnson RS. Isoforms of vascular endothelial growth factor act in a coordinate fashion to recruit and expand tumor vasculature. Molecular and Cellular Biology. 2000;20(19):7282–91. pmid:10982845
  17. 17. Lee S, Jilani SM, Nikolova GV, Carpizo D, Iruela-Arispe ML. Processing of VEGF-A by matrix metalloproteinases regulates bioavailability and vascular patterning in tumors. Journal of Cell Biology. 2005;169(4):681–91. pmid:15911882
  18. 18. Anderson SM, Shergill B, Barry ZT, Manousiouthakis E, Chen TT, Botvinick E, et al. VEGF internalization is not required for VEGFR-2 phosphorylation in bioengineered surfaces with covalently linked VEGF. Integrative Biology. 2011;3(9):887–96. pmid:21826315
  19. 19. Chen TT, Luque A, Lee S, Anderson SM, Segura T, Iruela-Arispe ML. Anchorage of VEGF to the extracellular matrix conveys differential signaling responses to endothelial cells. Journal of Cell Biology. 2010;188(4):595–609. pmid:20176926
  20. 20. Clegg LW, Mac Gabhann F. Site-Specific Phosphorylation of VEGFR2 Is Mediated by Receptor Trafficking: Insights from a Computational Model. PLoS Comput Biol. 2015;11(6):e1004158. pmid:26067165
  21. 21. Carmeliet P, Moons L, Luttun A, Vincenti V, Compernolle V, De Mol M, et al. Synergism between vascular endothelial growth factor and placental growth factor contributes to angiogenesis and plasma extravasation in pathological conditions. Nature Medicine. 2001;7(5):575–83. pmid:11329059
  22. 22. De Falco S. The discovery of placenta growth factor and its biological activity. Experimental and Molecular Medicine. 2012;44(1):1–9. pmid:22228176
  23. 23. Migdal M, Huppertz B, Tessler S, Comforti A, Shibuya M, Reich R, et al. Neuropilin-1 is a placenta growth factor-2 receptor. Journal of Biological Chemistry. 1998;273(35):22272–8. pmid:9712843
  24. 24. Yang W, Ahn H, Hinrichs M, Torry RJ, Torry DS. Evidence of a novel isoform of placenta growth factor (PlGF-4) expressed in human trophoblast and endothelial cells. Journal of Reproductive Immunology. 2003;60(1):53–60. pmid:14568677
  25. 25. Persico MG, Vincenti V, DiPalma T. Structure, expression and receptor-binding properties of placenta growth factor (PlGF). Vascular Growth Factors and Angiogenesis. 1999;237:31–40.
  26. 26. Dewerchin M, Carmeliet P. PlGF: A Multitasking Cytokine with Disease-Restricted Activity. Cold Spring Harbor Perspectives in Medicine. 2012;2(8).
  27. 27. Cao YH, Chen H, Zhou L, Chiang MK, AnandApte B, Weatherbee JA, et al. Heterodimers of placenta growth factor vascular endothelial growth factor—Endothelial activity, tumor cell expression, and high affinity binding to Flk-1/KDR. Journal of Biological Chemistry. 1996;271(6):3154–62. pmid:8621715
  28. 28. Eriksson A, Cao RH, Pawliuk R, Berg SM, Tsang M, Zhou D, et al. Placenta growth factor-1 antagonizes VEGF-induced angiogenesis and tumor growth by the formation of functionally inactive PlGF-1/VEGF heterodimers. Cancer Cell. 2002;1(1):99–108. pmid:12086892
  29. 29. Reuvekamp A, Velsing-Aarts FV, Poulina IEJ, Capello JJ, Duits AJ. Selective deficit of angiogenic growth factors characterises pregnancies complicated by pre-eclampsia. British Journal of Obstetrics and Gynaecology. 1999;106(10):1019–22. pmid:10519425
  30. 30. Livingston JC, Chin R, Haddad B, McKinney ET, Ahokas R, Sibai BM. Reductions of vascular endothelial growth factor and placental growth factor concentrations in severe preeclampsia. American Journal of Obstetrics and Gynecology. 2000;183(6):1554–7. pmid:11120527
  31. 31. Taylor RN, Grimwood J, Taylor RS, McMaster MT, Fisher SJ, North RA. Longitudinal serum concentrations of placental growth factor: Evidence for abnormal placental angiogenesis in pathologic pregnancies. American Journal of Obstetrics and Gynecology. 2003;188(1):177–82. pmid:12548214
  32. 32. Maynard SE, Min JY, Merchan J, Lim KH, Li JY, Mondal S, et al. Excess placental soluble fms-like tyrosine kinase 1 (sFlt1) may contribute to endothelial dysfimction, hypertension, and proteinuria in preeclampsia. Journal of Clinical Investigation. 2003;111(5):649–58. pmid:12618519
  33. 33. Madazli R, Aydin S, Uludag S, Vildan O, Tolun N. Maternal plasma levels of cytokines in normal and preeclamptic pregnancies and their relationship with diastolic blood pressure and fibronectin levels. Acta Obstetricia Et Gynecologica Scandinavica. 2003;82(9):797–802. pmid:12911439
  34. 34. Tsatsaris V, Goffin F, Munaut C, Brichant JFO, Pignon MR, Noel A, et al. Overexpression of the soluble vascular endothelial growth factor receptor in preeclamptic patients: Pathophysiological consequences. Journal of Clinical Endocrinology & Metabolism. 2003;88(11):5555–63.
  35. 35. Levine RJ, Maynard SE, Qian C, Lim KH, England LJ, Yu KF, et al. Circulating angiogenic factors and the risk of preeclampsia. New England Journal of Medicine. 2004;350(7):672–83. pmid:14764923
  36. 36. Muy-Rivera M, Vadachkoria S, Woelk GB, Qiu C, Mahomed K, Williams MA. Maternal plasma VEGF, sVEGF-R1, and PlGF concentrations in preeclamptic and normotensive pregnant Zimbabwean women. Physiological Research. 2005;54(6):611–22. pmid:15717861
  37. 37. Staff AC, Braekke K, Harsem NK, Lyberg T, Holthe MR. Circulating concentrations of sFlt1 (soluble fins-like tyrosine kinase 1) in fetal and maternal serum during pre-eclampsia. European Journal of Obstetrics Gynecology and Reproductive Biology. 2005;122(1):33–9.
  38. 38. Krauss T, Pauer HU, Augustin HG. Prospective analysis of placenta growth factor (PIGF) concentrations in the plasma of women with normal pregnancy and pregnancies complicated by preeclampsia. Hypertension in Pregnancy. 2004;23(1):101–11. pmid:15117604
  39. 39. D'Audigier C, Gautier B, Yon A, Alili JM, Evrard S, Inguimbert N, et al. Targeting VEGFR1 on endothelial progenitors modulates their differentiation potential. Journal of Thrombosis and Haemostasis. 2013;11:332-.
  40. 40. DePrimo SE, Bello CL, Smeraglia J, Baum CM, Spinella D, Rini BI, et al. Circulating protein biomarkers of pharmacodynamic activity of sunitinib in patients with metastatic renal cell carcinoma: modulation of VEGF and VEGF-related proteins. Journal of Translational Medicine. 2007;5.
  41. 41. Okamoto T, Saito C, Yamada S. Levels of placenta growth factor in gestational trophoblastic diseases. Placenta. 2004;25(10):A5–A.
  42. 42. Bates DO. An unexpected tail of VEGF and PlGF in pre-eclampsia. Biochemical Society Transactions. 2011;39:1576–82. pmid:22103490
  43. 43. Hiratsuka S, Minowa O, Kuno J, Noda T, Shibuya M. Flt-1 lacking the tyrosine kinase domain is sufficient for normal development and angiogenesis in mice. Proceedings of the National Academy of Sciences of the United States of America. 1998;95(16):9349–54. pmid:9689083
  44. 44. Autiero M, Waltenberger J, Communi D, Kranz A, Moons L, Lambrechts D, et al. Role of PIGF in the intra- and intermolecular cross talk between the VEGF receptors Flt1 and Flk1. Nature Medicine. 2003;9(7):936–43. pmid:12796773
  45. 45. Mac Gabhann F, Popel AS. Model of competitive binding of vascular endothelial growth factor and placental growth factor to VEGF receptors on endothelial cells. American Journal of Physiology-Heart and Circulatory Physiology. 2004;286(1).
  46. 46. Mac Gabhann F, Popel AS. Differential binding of VEGF isoforms to VEGF receptor 2 in the presence of neuropilin-1: a computational model. American Journal of Physiology-Heart and Circulatory Physiology. 2005;288(6):H2851–H60. pmid:15708957
  47. 47. Cebe-Suarez S, Zehnder-Fjallman A, Ballmer-Hofer K. The role of VEGF receptors in angiogenesis; complex partnerships. Cellular and Molecular Life Sciences. 2006;63(5):601–15. pmid:16465447
  48. 48. Park M, Lee ST. The fourth immunoglobulin-like loop in the extracellular domain of FLT-1, a VEGF receptor, includes a major heparin-binding site. Biochemical and Biophysical Research Communications. 1999;264(3):730–4. pmid:10544000
  49. 49. Orecchia A, Lacal PM, Schietroma C, Morea V, Zambruno G, Failla CM. Vascular endothelial growth factor receptor-1 is deposited in the extracellular matrix by endothelial cells and is a ligand for the alpha 5 beta 1 integrin. Journal of Cell Science. 2003;116(17):3479–89.
  50. 50. Kendall RL, Wang G, Thomas KA. Identification of a natural soluble form of the vascular endothelial growth factor receptor, FLT-1, and its heterodimerization with KDR. Biochemical and Biophysical Research Communications. 1996;226(2):324–8. pmid:8806634
  51. 51. Rossi A, Gauvrit S, Marass M, Pan LY, Moens CB, Stainier DYR. Regulation of Vegf signaling by natural and synthetic ligands. Blood. 2016;128(19):2359–66.
  52. 52. Tjwa M, Luttun A, Autiero M, Carmeliet P. VEGF and PlGF: two pleiotropic growth factors with distinct roles in development and homeostasis. Cell and Tissue Research. 2003;314(1):5–14. pmid:13680354
  53. 53. Park JE, Chen HH, Winer J, Houck KA, Ferrara N. Placenta growth-factor—Potentiation of Vascular Endothelial Growth-Factor Bioactivity, in-vitro and in-vivo, and high-affinity binding to the FLT-1 but not to FLK-1/KDR. Journal of Biological Chemistry. 1994;269(41):25646–54. pmid:7929268
  54. 54. Robciuc MR, Kivela R, Williams IM, de Boer JF, van Dijk TH, Elamaa H, et al. VEGFB/VEGFR1-Induced Expansion of Adipose Vasculature Counteracts Obesity and Related Metabolic Complications. Cell Metabolism. 2016;23(4):712–24. pmid:27076080
  55. 55. Clegg LE, Mac Gabhann F. Molecular mechanism matters: Benefits of mechanistic computational models for drug development. Pharmacological Research. 2015;99(0):149–54.
  56. 56. Stefanini MO, Wu FT, Mac Gabhann F, Popel AS. A compartment model of VEGF distribution in blood, healthy and diseased tissues. BMC Systems Biology. 2008;2.
  57. 57. Wu FTH, Stefanini MO, Gabhann FM, Popel AS. A Compartment Model of VEGF Distribution in Humans in the Presence of Soluble VEGF Receptor-1 Acting as a Ligand Trap. Plos One. 2009;4(4).
  58. 58. Wu FT, Stefanini MO, Mac Gabhann F, Kontos CD, Annex BH, Popel AS. VEGF and soluble VEGF receptor-1 (sFlt-1) distributions in peripheral arterial disease: an in silico model. Am J Physiol Heart Circ Physiol. 2010;298(6):H2174–91. Epub 2010/04/13. pmid:20382861
  59. 59. Finley SD, Popel AS. Effect of Tumor Microenvironment on Tumor VEGF During Anti-VEGF Treatment: Systems Biology Predictions. Jnci-Journal of the National Cancer Institute. 2013;105(11):802–11.
  60. 60. Stefanini MO, Wu FTH, Mac Gabhann F, Popel AS. Increase of Plasma VEGF after Intravenous Administration of Bevacizumab Is Predicted by a Pharmacokinetic Model. Cancer Research. 2010;70(23):9886–94. pmid:21118974
  61. 61. Finley SD, Dhar M, Popel AS. Compartment model predicts VEGF secretion and investigates the effects of VEGF trap in tumor-bearing mice. Frontiers in oncology. 2013;3:196-. pmid:23908970
  62. 62. Yen P, Finley SD, Engel-Stefanini MO, Popel AS. A Two-Compartment Model of VEGF Distribution in the Mouse. Plos One. 2011;6(11).
  63. 63. Imoukhuede PI, Popel AS. Quantification and cell-to-cell variation of vascular endothelial growth factor receptors. Experimental Cell Research. 2011;317(7):955–65. pmid:21185287
  64. 64. Vintonenko N, Pelaez-Garavito I, Buteau-Lozano H, Toullec A, Lidereau R, Perret GY, et al. Overexpression of VEGF189 in breast cancer cells induces apoptosis via NRP1 under stress conditions. Cell Adhesion & Migration. 2011;5(4):332–43.
  65. 65. Hoffmann DC, Willenborg S, Koch M, Zwolanek D, Mueller S, Becker A-KA, et al. Proteolytic Processing Regulates Placental Growth Factor Activities. Journal of Biological Chemistry. 2013;288(25):17976–89. pmid:23645683
  66. 66. Martino MM, Briquez PS, Güç E, Tortelli F, Kilarski WW, Metzger S, et al. Growth Factors Engineered for Super-Affinity to the Extracellular Matrix Enhance Tissue Healing. Science. 2014;343(6173):885–8. pmid:24558160
  67. 67. Imoukhuede PI, Popel AS. Expression of VEGF Receptors on Endothelial Cells in Mouse Skeletal Muscle. Plos One. 2012;7(9).
  68. 68. Nucci M, Poon LC, Demirdjian G, Darbouret B, Nicolaides KH. Maternal Serum Placental Growth Factor (PIGF) Isoforms 1 and 2 at 11–13 Weeks' Gestation in Normal and Pathological Pregnancies. Fetal Diagnosis and Therapy. 2014;36(2):106–16. pmid:24457972
  69. 69. Ng YS, Rohan R, Sunday ME, Demello DE, D'Amore PA. Differential expression of VEGF isoforms in mouse during development and in the adult. Developmental Dynamics. 2001;220(2):112–21. pmid:11169844
  70. 70. Wu FTH, Stefanini MO, Mac Gabhann F, Kontos CD, Annex BH, Popel AS. A systems biology perspective on sVEGFR1: its biological function, pathogenic role and therapeutic use. Journal of Cellular and Molecular Medicine. 2010;14(3):528–52. pmid:19840194
  71. 71. Fuh G, Garcia KC, de Vos AM. The interaction of neuropilin-1 with vascular endothelial growth factor and its receptor Flt-1. Journal of Biological Chemistry. 2000;275(35):26690–5. pmid:10842181
  72. 72. Pan Q, Chathery Y, Wu Y, Rathore N, Tong RK, Peale F, et al. Neuropilin-1 binds to VEGF(121) and regulates endothelial cell migration and sprouting. Journal of Biological Chemistry. 2007;282(33):24049–56. pmid:17575273
  73. 73. Hu S, Sun Y, Meng Y, Wang X, Yang W, Fu W, et al. Molecular architecture of the ErbB2 extracellular domain homodimer. Oncotarget. 2015;6(3):1695–706. pmid:25633808
  74. 74. Cho HS, Leahy DJ. Structure of the extracellular region of HER3 reveals an interdomain tether. Science. 2002;297(5585):1330–3. pmid:12154198
  75. 75. Cho HS, Mason K, Ramyar KX, Stanley AM, Gabelli SB, Denney DW, et al. Structure of the extracellular region of HER2 alone and in complex with the Herceptin Fab. Nature. 2003;421(6924):756–60. pmid:12610629
  76. 76. Bruns AF, Bao L, Walker JH, Ponnambalam S. VEGF-A-stimulated signalling in endothelial cells via a dual receptor tyrosine kinase system is dependent on co-ordinated trafficking and proteolysis. Biochemical Society Transactions. 2009;37:1193–7. pmid:19909245
  77. 77. Mittar S, Ulyatt C, Howell GJ, Bruns AF, Zachary I, Walker JH, et al. VEGFR1 receptor tyrosine kinase localization to the Golgi apparatus is calcium-dependent. Experimental Cell Research. 2009;315(5):877–89. pmid:19162007
  78. 78. Filion RJ, Popel AS. A reaction-diffusion model of basic fibroblast growth factor interactions with cell surface receptors. Annals of Biomedical Engineering. 2004;32(5):645–63. pmid:15171620
  79. 79. Mac Gabhann F, Popel AS. Interactions of VEGF isoforms with VEGFR-1, VEGFR-2, and neuropilin in vivo: a computational model of human skeletal muscle. American Journal of Physiology-Heart and Circulatory Physiology. 2007;292(1).
  80. 80. Rohrbach DH, Wagner CW, Star VL, Martin GR, Brown KS, Yoon JW. Reduced synthesis of basement-membrane heparan-sulfate proteoglycans in streptozotocin-induced diabetic mice. Journal of Biological Chemistry. 1983;258(19):1672–7.
  81. 81. Yamamoto H, Rundqvist H, Branco C, Johnson RS. Autocrine VEGF Isoforms Differentially Regulate Endothelial Cell Behavior. Frontiers in Cell and Developmental Biology. 2016;4(99).
  82. 82. Carmeliet P, Ng YS, Nuyens D, Theilmeier G, Brusselmans K, Cornelissen I, et al. Impaired myocardial angiogenesis and ischemic cardiomyopathy in mice lacking the vascular endothelial growth factor isoforms VEGF(164) and VEGF(188). Nature Medicine. 1999;5(5):495–502. pmid:10229225
  83. 83. Pipp F, Heil M, Issbrucker K, Ziegelhoeffer T, Martin S, van den Heuvel J, et al. VEGFR-1-selective VEGF homologue PlGF is arteriogenic—Evidence for a monocyte-mediated mechanism. Circulation Research. 2003;92(4):378–85. pmid:12600898
  84. 84. Escudero-Esparza A, Martin TA, Douglas-Jones A, Mansel RE, Jiang WG. PGF isoforms, PLGF-1 and PGF-2 and the PGF receptor, neuropilin, in human breast cancer: Prognostic significance. Oncology Reports. 2010;23(2):537–44. pmid:20043119
  85. 85. Marcellini M, De Luca N, Riccioni T, Ciucci A, Orecchia A, Lacal PM, et al. Increased melanoma growth and metastasis spreading in mice overexpressing placenta growth factor. American Journal of Pathology. 2006;169(2):643–54. pmid:16877362
  86. 86. Roy H, Bhardwaj S, Babu M, Jauhiainen S, Herzig KH, Bellu AR, et al. Adenovirus-mediated gene transfer of placental growth factor to perivascular tissue induces angiogenesis via upregulation of the expression of endogenous vascular endothelial growth factor-A. Human Gene Therapy. 2005;16(12):1422–8. pmid:16390273
  87. 87. Räsänen M, Degerman J, Nissinen TA, Miinalainen I, Kerkelä R, Siltanen A, et al. VEGF-B gene therapy inhibits doxorubicin-induced cardiotoxicity by endothelial protection. Proceedings of the National Academy of Sciences. 2016;113(46):13144–9.
  88. 88. Hazarika S, Dokun AO, Li Y, Popel AS, Kontos CD, Annex BH. Impaired angiogenesis after Hindlimb ischemia in type 2 diabetes Mellitus—Differential regulation of vascular endothelial growth factor receptor 1 and soluble vascular endothelial growth factor receptor 1. Circulation Research. 2007;101(9):948–56. pmid:17823371
  89. 89. Martino MM, Tortelli F, Mochizuki M, Traub S, Ben-David D, Kuhn GA, et al. Engineering the Growth Factor Microenvironment with Fibronectin Domains to Promote Wound and Bone Tissue Healing. Science Translational Medicine. 2011;3(100).
  90. 90. Jakobsson L, Kreuger J, Holmborn K, Lundin L, Eriksson I, Kjellen L, et al. Heparan sulfate in trans potentiates VEGFR-mediated angiogenesis. Developmental Cell. 2006;10(5):625–34. pmid:16678777
  91. 91. Koch S, van Meeteren LA, Morin E, Testini C, Westrom S, Bjorkelund H, et al. NRP1 Presented in trans to the Endothelium Arrests VEGFR2 Endocytosis, Preventing Angiogenic Signaling and Tumor Initiation. Developmental Cell. 2014;28(6):633–46. pmid:24656741
  92. 92. 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. pmid:7596436
  93. 93. Bussolati B, Dunk C, Grohman M, Kontos CD, Mason J, Ahmed A. Vascular endothelial growth factor receptor-1 modulates vascular endothelial growth factor-mediated angiogenesis via nitric oxide. American Journal of Pathology. 2001;159(3):993–1008. pmid:11549592
  94. 94. Kikuchi R, Nakamura K, MacLauchlan S, Doan Thi-Minh N, Shimizu I, Fuster JJ, et al. An antiangiogenic isoform of VEGF-A contributes to impaired vascularization in peripheral artery disease. Nature Medicine. 2014;20(12):1464–71. pmid:25362254
  95. 95. Ngo DTM, Farb MG, Kikuchi R, Karki S, Tiwari S, Bigornia SJ, et al. Antiangiogenic Actions of Vascular Endothelial Growth Factor-A(165)b, an Inhibitory Isoform of Vascular Endothelial Growth Factor-A, in Human Obesity. Circulation. 2014;130(13):1072–80. pmid:25116954
  96. 96. Vempati P, Mac Gabhann F, Popel AS. Quantifying the Proteolytic Release of Extracellular Matrix-Sequestered VEGF with a Computational Model. Plos One. 2010;5(7).
  97. 97. Vempati P, Popel AS, Mac Gabhann F. Formation of VEGF isoform-specific spatial distributions governing angiogenesis: computational analysis. BMC Syst Biol. 2011;5:59. Epub 2011/05/04. pmid:21535871
  98. 98. Chappell JC, Cluceru JG, Nesmith JE, Mouillesseaux KP, Bradley VB, Hartland CM, et al. Flt-1 (VEGFR-1) coordinates discrete stages of blood vessel formation. Cardiovascular Research. 2016;111(1):84–93. pmid:27142980
  99. 99. Hashambhoy YL, Chappell JC, Peirce SM, Bautch VL, Mac Gabhann F. Computational modeling of interacting VEGF and soluble VEGF receptor concentration gradients. Front Physiol. 2011;2:62. Epub 2011/10/19. pmid:22007175
  100. 100. Ji JW, Mac Gabhann F, Popel AS. Skeletal muscle VEGF gradients in peripheral arterial disease: Simulations of rest and exercise. Am J Physiol Heart Circ Physiol. 2007;293:H3740–H9. pmid:17890434
  101. 101. Vempati P, Popel AS, Mac Gabhann F. Formation of VEGF isoform-specific spatial distributions governing angiogenesis: computational analysis. BMC Systems Biology. 2011;5.