Abstract
Pericytes are vascular mural cells embedded in the basement membrane of blood microvessels. They extend their processes along capillaries, pre-capillary arterioles and post-capillary venules. CNS pericytes are uniquely positioned in the neurovascular unit between endothelial cells, astrocytes and neurons. They integrate, coordinate and process signals from their neighboring cells to generate diverse functional responses that are critical for CNS functions in health and disease, including regulation of the blood–brain barrier permeability, angiogenesis, clearance of toxic metabolites, capillary hemodynamic responses, neuroinflammation and stem cell activity. Here we examine the key signaling pathways between pericytes and their neighboring endothelial cells, astrocytes and neurons that control neurovascular functions. We also review the role of pericytes in CNS disorders including rare monogenic diseases and complex neurological disorders such as Alzheimer's disease and brain tumors. Finally, we discuss directions for future studies.
This is a preview of subscription content, access via your institution
Access options
Subscribe to this journal
Receive 12 print issues and online access
$209.00 per year
only $17.42 per issue
Buy this article
- Purchase on SpringerLink
- Instant access to full article PDF
Prices may be subject to local taxes which are calculated during checkout
Similar content being viewed by others
References
Zlokovic, B.V. Neurovascular pathways to neurodegeneration in Alzheimer's disease and other disorders. Nat. Rev. Neurosci. 12, 723–738 (2011).
Winkler, E.A., Bell, R.D. & Zlokovic, B.V. Central nervous system pericytes in health and disease. Nat. Neurosci. 14, 1398–1405 (2011).
Iadecola, C. The pathobiology of vascular dementia. Neuron 80, 844–866 (2013).
Attwell, D. et al. Glial and neuronal control of brain blood flow. Nature 468, 232–243 (2010).
Armulik, A., Genové, G. & Betsholtz, C. Pericytes: developmental, physiological, and pathological perspectives, problems, and promises. Dev. Cell 21, 193–215 (2011).
Hamilton, N.B., Attwell, D. & Hall, C.N. Pericyte-mediated regulation of capillary diameter: a component of neurovascular coupling in health and disease. Front. Neuroenergetics http://dx.doi.org/10.3389/fnene.2010.00005 (2010).
Zhao, Z., Nelson, A.R., Betsholtz, C. & Zlokovic, B.V. Establishment and dysfunction of the blood-brain barrier. Cell 163, 1064–1078 (2015).
Daneman, R., Zhou, L., Kebede, A.A. & Barres, B.A. Pericytes are required for blood-brain barrier integrity during embryogenesis. Nature 468, 562–566 (2010).
Armulik, A. et al. Pericytes regulate the blood-brain barrier. Nature 468, 557–561 (2010).
Bell, R.D. et al. Pericytes control key neurovascular functions and neuronal phenotype in the adult brain and during brain aging. Neuron 68, 409–427 (2010).
Bell, R.D. et al. Apolipoprotein E controls cerebrovascular integrity via cyclophilin A. Nature 485, 512–516 (2012).
Zlokovic, B.V., Begley, D.J. & Chain-Eliash, D.G. Blood-brain barrier permeability to leucine-enkephalin, D-alanine2-D-leucine5-enkephalin and their N-terminal amino acid (tyrosine). Brain Res. 336, 125–132 (1985).
Zlokovic´, B.V., Segal, M.B., Begley, D.J., Davson, H. & Rakic´, L. Permeability of the blood-cerebrospinal fluid and blood-brain barriers to thyrotropin-releasing hormone. Brain Res. 358, 191–199 (1985).
Zlokovic´, B.V., Lipovac, M.N., Begley, D.J., Davson, H. & Rakic´, L. Transport of leucine-enkephalin across the blood-brain barrier in the perfused guinea pig brain. J. Neurochem. 49, 310–315 (1987).
Zlokovic, B.V. Cerebrovascular permeability to peptides: manipulations of transport systems at the blood-brain barrier. Pharm. Res. 12, 1395–1406 (1995).
Zlokovic, B.V. Neurodegeneration and the neurovascular unit. Nat. Med. 16, 1370–1371 (2010).
Dore-Duffy, P. Pericytes: pluripotent cells of the blood brain barrier. Curr. Pharm. Des. 14, 1581–1593 (2008).
Krueger, M. & Bechmann, I. CNS pericytes: concepts, misconceptions, and a way out. Glia 58, 1–10 (2010).
Attwell, D., Mishra, A., Hall, C.N., O'Farrell, F.M. & Dalkara, T. What is a pericyte? J. Cereb. Blood Flow Metab. 36, 451–455 (2016).
Hartmann, D.A. et al. Pericyte structure and distribution in the cerebral cortex revealed by high-resolution imaging of transgenic mice. Neurophotonics 2, 041402 (2015).
van Dijk, C.G.M. et al. The complex mural cell: pericyte function in health and disease. Int. J. Cardiol. 190, 75–89 (2015).
Bondjers, C. et al. Microarray analysis of blood microvessels from PDGF-B and PDGF-Rbeta mutant mice identifies novel markers for brain pericytes. FASEB J. 20, 1703–1705 (2006).
Johnson, M.B. et al. Single-cell analysis reveals transcriptional heterogeneity of neural progenitors in human cortex. Nat. Neurosci. 18, 637–646 (2015).
Kim, K.-T. et al. Single-cell mRNA sequencing identifies subclonal heterogeneity in anti-cancer drug responses of lung adenocarcinoma cells. Genome Biol. 16, 127 (2015).
Arnold, T.D. et al. Excessive vascular sprouting underlies cerebral hemorrhage in mice lacking αVβ8-TGFβ signaling in the brain. Development 141, 4489–4499 (2014).
Sagare, A.P. et al. Pericyte loss influences Alzheimer-like neurodegeneration in mice. Nat. Commun. 4, 2932 (2013).
Pieper, C., Marek, J.J., Unterberg, M., Schwerdtle, T. & Galla, H.-J. Brain capillary pericytes contribute to the immune defense in response to cytokines or LPS in vitro. Brain Res. 1550, 1–8 (2014).
Iadecola, C. & Nedergaard, M. Glial regulation of the cerebral microvasculature. Nat. Neurosci. 10, 1369–1376 (2007).
MacVicar, B.A. & Newman, E.A. Astrocyte regulation of blood flow in the brain. Cold Spring Harb. Perspect. Biol. 7, a020388 (2015).
Hall, C.N. et al. Capillary pericytes regulate cerebral blood flow in health and disease. Nature 508, 55–60 (2014).
Fernández-Klett, F., Offenhauser, N., Dirnagl, U., Priller, J. & Lindauer, U. Pericytes in capillaries are contractile in vivo, but arterioles mediate functional hyperemia in the mouse brain. Proc. Natl. Acad. Sci. USA 107, 22290–22295 (2010).
Dai, M., Nuttall, A., Yang, Y. & Shi, X. Visualization and contractile activity of cochlear pericytes in the capillaries of the spiral ligament. Hear. Res. 254, 100–107 (2009).
Yamanishi, S., Katsumura, K., Kobayashi, T. & Puro, D.G. Extracellular lactate as a dynamic vasoactive signal in the rat retinal microvasculature. Am. J. Physiol. Heart Circ. Physiol. 290, H925–H934 (2006).
Chaigneau, E., Oheim, M., Audinat, E. & Charpak, S. Two-photon imaging of capillary blood flow in olfactory bulb glomeruli. Proc. Natl. Acad. Sci. USA 100, 13081–13086 (2003).
Peppiatt, C.M., Howarth, C., Mobbs, P. & Attwell, D. Bidirectional control of CNS capillary diameter by pericytes. Nature 443, 700–704 (2006).
Hill, R.A. et al. Regional blood flow in the normal and ischemic brain is controlled by arteriolar smooth muscle cell contractility and not by capillary pericytes. Neuron 87, 95–110 (2015).
Olson, L.E. & Soriano, P. PDGFRβ signaling regulates mural cell plasticity and inhibits fat development. Dev. Cell 20, 815–826 (2011).
Wang, S. et al. Venular basement membranes contain specific matrix protein low expression regions that act as exit points for emigrating neutrophils. J. Exp. Med. 203, 1519–1532 (2006).
Voisin, M.-B., Pröbstl, D. & Nourshargh, S. Venular basement membranes ubiquitously express matrix protein low-expression regions: characterization in multiple tissues and remodeling during inflammation. Am. J. Pathol. 176, 482–495 (2010).
Jansson, D. et al. A role for human brain pericytes in neuroinflammation. J. Neuroinflammation 11, 104 (2014).
Kovac, A., Erickson, M.A. & Banks, W.A. Brain microvascular pericytes are immunoactive in culture: cytokine, chemokine, nitric oxide, and LRP-1 expression in response to lipopolysaccharide. J. Neuroinflammation 8, 139 (2011).
Nakagomi, T. et al. Brain vascular pericytes following ischemia have multipotential stem cell activity to differentiate into neural and vascular lineage cells. Stem Cells 33, 1962–1974 (2015).
Winkler, E.A., Sengillo, J.D., Bell, R.D., Wang, J. & Zlokovic, B.V. Blood-spinal cord barrier pericyte reductions contribute to increased capillary permeability. J. Cereb. Blood Flow Metab. 32, 1841–1852 (2012).
Winkler, E.A. et al. Blood-spinal cord barrier disruption contributes to early motor-neuron degeneration in ALS-model mice. Proc. Natl. Acad. Sci. USA 111, E1035–E1042 (2014).
Davalos, D. et al. Fibrinogen-induced perivascular microglial clustering is required for the development of axonal damage in neuroinflammation. Nat. Commun. 3, 1227 (2012).
Yemisci, M. et al. Pericyte contraction induced by oxidative-nitrative stress impairs capillary reflow despite successful opening of an occluded cerebral artery. Nat. Med. 15, 1031–1037 (2009).
Keller, A. et al. Mutations in the gene encoding PDGF-B cause brain calcifications in humans and mice. Nat. Genet. 45, 1077–1082 (2013).
Nicolas, G. et al. Mutation of the PDGFRB gene as a cause of idiopathic basal ganglia calcification. Neurology 80, 181–187 (2013).
Halliday, M.R. et al. Relationship between cyclophilin a levels and matrix metalloproteinase 9 activity in cerebrospinal fluid of cognitively normal apolipoprotein e4 carriers and blood-brain barrier breakdown. JAMA Neurol. 70, 1198–1200 (2013).
Halliday, M.R. et al. Accelerated pericyte degeneration and blood-brain barrier breakdown in apolipoprotein E4 carriers with Alzheimer's disease. J. Cereb. Blood Flow Metab. http://dx.doi.org/10.1038/jcbfm.2015.44 (2015).10.1038/jcbfm.2015.44
Winkler, E.A. et al. Blood-spinal cord barrier breakdown and pericyte reductions in amyotrophic lateral sclerosis. Acta Neuropathol. 125, 111–120 (2013).
Geraldes, P. et al. Activation of PKC-delta and SHP-1 by hyperglycemia causes vascular cell apoptosis and diabetic retinopathy. Nat. Med. 15, 1298–1306 (2009).
Behl, Y., Krothapalli, P., Desta, T., Roy, S. & Graves, D.T. FOXO1 plays an important role in enhanced microvascular cell apoptosis and microvascular cell loss in type 1 and type 2 diabetic rats. Diabetes 58, 917–925 (2009).
Alikhani, M., Roy, S. & Graves, D.T. FOXO1 plays an essential role in apoptosis of retinal pericytes. Mol. Vis. 16, 408–415 (2010).
Niu, F., Yao, H., Zhang, W., Sutliff, R.L. & Buch, S. Tat 101-mediated enhancement of brain pericyte migration involves platelet-derived growth factor subunit B homodimer: implications for human immunodeficiency virus-associated neurocognitive disorders. J. Neurosci. 34, 11812–11825 (2014).
Marchi, N. & Lerner-Natoli, M. Cerebrovascular remodeling and epilepsy. Neuroscientist 19, 304–312 (2013).
Ghosh, M. et al. Pericytes are involved in the pathogenesis of CADASIL. Ann. Neurol. 78, 887–900 (2015).
Wang, F. et al. A microRNA-1280/JAG2 network comprises a novel biological target in high-risk medulloblastoma. Oncotarget 6, 2709–2724 (2015).
Heldin, C.-H. Targeting the PDGF signaling pathway in tumor treatment. Cell Commun. Signal. 11, 97 (2013).
Lindahl, P., Johansson, B.R., Levéen, P. & Betsholtz, C. Pericyte loss and microaneurysm formation in PDGF-B-deficient mice. Science 277, 242–245 (1997).
Winkler, E.A., Bell, R.D. & Zlokovic, B.V. Pericyte-specific expression of PDGF beta receptor in mouse models with normal and deficient PDGF beta receptor signaling. Mol. Neurodegener. 5, 32 (2010).
Tallquist, M.D., French, W.J. & Soriano, P. Additive effects of PDGF receptor beta signaling pathways in vascular smooth muscle cell development. PLoS Biol. 1, e52 (2003).
Jurek, A., Heldin, C.-H. & Lennartsson, J. Platelet-derived growth factor-induced signaling pathways interconnect to regulate the temporal pattern of Erk1/2 phosphorylation. Cell. Signal. 23, 280–287 (2011).
Jin, S. et al. Notch signaling regulates platelet-derived growth factor receptor-beta expression in vascular smooth muscle cells. Circ. Res. 102, 1483–1491 (2008).
Song, S., Ewald, A.J., Stallcup, W., Werb, Z. & Bergers, G. PDGFRbeta+ perivascular progenitor cells in tumours regulate pericyte differentiation and vascular survival. Nat. Cell Biol. 7, 870–879 (2005).
Hellström, M. et al. Lack of pericytes leads to endothelial hyperplasia and abnormal vascular morphogenesis. J. Cell Biol. 153, 543–553 (2001).
Wang, C. et al. Mutations in SLC20A2 link familial idiopathic basal ganglia calcification with phosphate homeostasis. Nat. Genet. 44, 254–256 (2012).
Lemos, R.R. et al. Update and mutational analysis of SLC20A2: a major cause of primary familial brain calcification. Hum. Mutat. 36, 489–495 (2015).
Sengillo, J.D. et al. Deficiency in mural vascular cells coincides with blood-brain barrier disruption in Alzheimer's disease. Brain Pathol. 23, 303–310 (2013).
Farkas, E. & Luiten, P.G. Cerebral microvascular pathology in aging and Alzheimer's disease. Prog. Neurobiol. 64, 575–611 (2001).
Baloyannis, S.J. & Baloyannis, I.S. The vascular factor in Alzheimer's disease: a study in Golgi technique and electron microscopy. J. Neurol. Sci. 322, 117–121 (2012).
Park, L. et al. Innate immunity receptor CD36 promotes cerebral amyloid angiopathy. Proc. Natl. Acad. Sci. USA 110, 3089–3094 (2013).
Montagne, A. et al. Blood-brain barrier breakdown in the aging human hippocampus. Neuron 85, 296–302 (2015).
Björkqvist, M., Ohlsson, M., Minthon, L. & Hansson, O. Evaluation of a previously suggested plasma biomarker panel to identify Alzheimer's disease. PLoS One 7, e29868 (2012).
Sagare, A.P., Sweeney, M.D., Makshanoff, J. & Zlokovic, B.V. Shedding of soluble platelet-derived growth factor receptor-β from human brain pericytes. Neurosci. Lett. 607, 97–101 (2015).
Rogaeva, E. et al. The neuronal sortilin-related receptor SORL1 is genetically associated with Alzheimer disease. Nat. Genet. 39, 168–177 (2007).
Reitz, C. et al. Meta-analysis of the association between variants in SORL1 and Alzheimer disease. Arch. Neurol. 68, 99–106 (2011).
Kooner, J.S. et al. Genome-wide association study in individuals of South Asian ancestry identifies six new type 2 diabetes susceptibility loci. Nat. Genet. 43, 984–989 (2011).
Reitz, C. The role of intracellular trafficking and the VPS10d receptors in Alzheimer's disease. Future Neurol. 7, 423–431 (2012).
Hermey, G., Sjøgaard, S.S., Petersen, C.M., Nykjaer, A. & Gliemann, J. Tumour necrosis factor alpha-converting enzyme mediates ectodomain shedding of Vps10p-domain receptor family members. Biochem. J. 395, 285–293 (2006).
Gliemann, J. et al. The mosaic receptor sorLA/LR11 binds components of the plasminogen-activating system and platelet-derived growth factor-BB similarly to LRP1 (low-density lipoprotein receptor-related protein), but mediates slow internalization of bound ligand. Biochem. J. 381, 203–212 (2004).
Zlokovic, B.V., Deane, R., Sagare, A.P., Bell, R.D. & Winkler, E.A. Low-density lipoprotein receptor-related protein-1: a serial clearance homeostatic mechanism controlling Alzheimer's amyloid β-peptide elimination from the brain. J. Neurochem. 115, 1077–1089 (2010).
Karch, C.M., Cruchaga, C. & Goate, A.M. Alzheimer's disease genetics: from the bench to the clinic. Neuron 83, 11–26 (2014).
Armstrong, R.A. Spatial correlations between beta-amyloid (Abeta) deposits and blood vessels in familial Alzheimer's disease. Folia Neuropathol. 46, 241–248 (2008).
Kang, D.E. et al. Presenilins mediate phosphatidylinositol 3-kinase/AKT and ERK activation via select signaling receptors. Selectivity of PS2 in platelet-derived growth factor signaling. J. Biol. Chem. 280, 31537–31547 (2005).
Gama Sosa, M.A. et al. Age-related vascular pathology in transgenic mice expressing presenilin 1-associated familial Alzheimer's disease mutations. Am. J. Pathol. 176, 353–368 (2010).
Sweeney, M.D., Sagare, A.P. & Zlokovic, B.V. Cerebrospinal fluid biomarkers of neurovascular dysfunction in mild dementia and Alzheimer's disease. J. Cereb. Blood Flow Metab. 35, 1055–1068 (2015).
Zhong, Z. et al. ALS-causing SOD1 mutants generate vascular changes prior to motor neuron degeneration. Nat. Neurosci. 11, 420–422 (2008).
DeJesus-Hernandez, M. et al. Expanded GGGGCC hexanucleotide repeat in noncoding region of C9ORF72 causes chromosome 9p-linked FTD and ALS. Neuron 72, 245–256 (2011).
Bergers, G., Song, S., Meyer-Morse, N., Bergsland, E. & Hanahan, D. Benefits of targeting both pericytes and endothelial cells in the tumor vasculature with kinase inhibitors. J. Clin. Invest. 111, 1287–1295 (2003).
Shaheen, R.M. et al. Tyrosine kinase inhibition of multiple angiogenic growth factor receptors improves survival in mice bearing colon cancer liver metastases by inhibition of endothelial cell survival mechanisms. Cancer Res. 61, 1464–1468 (2001).
Guichet, P.-O. et al. Notch1 stimulation induces a vascularization switch with pericyte-like cell differentiation of glioblastoma stem cells. Stem Cells 33, 21–34 (2015).
Cheng, L. et al. Glioblastoma stem cells generate vascular pericytes to support vessel function and tumor growth. Cell 153, 139–152 (2013).
Sato, Y. & Rifkin, D.B. Inhibition of endothelial cell movement by pericytes and smooth muscle cells: activation of a latent transforming growth factor-beta 1-like molecule by plasmin during co-culture. J. Cell Biol. 109, 309–315 (1989).
Hirschi, K.K., Burt, J.M., Hirschi, K.D. & Dai, C. Gap junction communication mediates transforming growth factor-beta activation and endothelial-induced mural cell differentiation. Circ. Res. 93, 429–437 (2003).
Van Geest, R.J., Klaassen, I., Vogels, I.M.C., Van Noorden, C.J.F. & Schlingemann, R.O. Differential TGF-beta signaling in retinal vascular cells: a role in diabetic retinopathy? Invest. Ophthalmol. Vis. Sci. 51, 1857–1865 (2010).
Reyahi, A. et al. Foxf2 is required for brain pericyte differentiation and development and maintenance of the blood-brain barrier. Dev. Cell 34, 19–32 (2015).
Darland, D.C. & D'Amore, P.A. TGF beta is required for the formation of capillary-like structures in three-dimensional cocultures of 10T1/2 and endothelial cells. Angiogenesis 4, 11–20 (2001).
Maddaluno, L. et al. EndMT contributes to the onset and progression of cerebral cavernous malformations. Nature 498, 492–496 (2013).
Li, F. et al. Endothelial Smad4 maintains cerebrovascular integrity by activating N-cadherin through cooperation with Notch. Dev. Cell 20, 291–302 (2011).
Goumans, M.J. & Mummery, C. Functional analysis of the TGFbeta receptor/Smad pathway through gene ablation in mice. Int. J. Dev. Biol. 44, 253–265 (2000).
Vinukonda, G. et al. Effect of prenatal glucocorticoids on cerebral vasculature of the developing brain. Stroke 41, 1766–1773 (2010).
Schulz, G.B. et al. Cerebral cavernous malformation-1 protein controls DLL4-Notch3 signaling between the endothelium and pericytes. Stroke 46, 1337–1343 (2015).
Bergametti, F. et al. Mutations within the programmed cell death 10 gene cause cerebral cavernous malformations. Am. J. Hum. Genet. 76, 42–51 (2005).
Li, X. et al. Molecular recognition of leucine-aspartate repeat (LD) motifs by the focal adhesion targeting homology domain of cerebral cavernous malformation 3 (CCM3). J. Biol. Chem. 286, 26138–26147 (2011).
Bruna, A. et al. High TGFbeta-Smad activity confers poor prognosis in glioma patients and promotes cell proliferation depending on the methylation of the PDGF-B gene. Cancer Cell 11, 147–160 (2007).
Dieterich, L.C. et al. Transcriptional profiling of human glioblastoma vessels indicates a key role of VEGF-A and TGFβ2 in vascular abnormalization. J. Pathol. 228, 378–390 (2012).
Svensson, A., Özen, I., Genové, G., Paul, G. & Bengzon, J. Endogenous brain pericytes are widely activated and contribute to mouse glioma microvasculature. PLoS One 10, e0123553 (2015).
Slevin, M. et al. Serial measurement of vascular endothelial growth factor and transforming growth factor-beta1 in serum of patients with acute ischemic stroke. Stroke 31, 1863–1870 (2000).
Böttner, M., Krieglstein, K. & Unsicker, K. The transforming growth factor-betas: structure, signaling, and roles in nervous system development and functions. J. Neurochem. 75, 2227–2240 (2000).
Henshall, T.L. et al. Notch3 is necessary for blood vessel integrity in the central nervous system. Arterioscler. Thromb. Vasc. Biol. 35, 409–420 (2015).
Reis, M. & Liebner, S. Wnt signaling in the vasculature. Exp. Cell Res. 319, 1317–1323 (2013).
Liebner, S. & Plate, K.H. Differentiation of the brain vasculature: the answer came blowing by the Wnt. J. Angiogenes. Res. 2, 1 (2010).
Ruhrberg, C. et al. Spatially restricted patterning cues provided by heparin-binding VEGF-A control blood vessel branching morphogenesis. Genes Dev. 16, 2684–2698 (2002).
Gerhardt, H. et al. VEGF guides angiogenic sprouting utilizing endothelial tip cell filopodia. J. Cell Biol. 161, 1163–1177 (2003).
Hellström, M. et al. Dll4 signalling through Notch1 regulates formation of tip cells during angiogenesis. Nature 445, 776–780 (2007).
Gale, N.W. et al. Haploinsufficiency of delta-like 4 ligand results in embryonic lethality due to major defects in arterial and vascular development. Proc. Natl. Acad. Sci. USA 101, 15949–15954 (2004).
Krebs, L.T. et al. Haploinsufficient lethality and formation of arteriovenous malformations in Notch pathway mutants. Genes Dev. 18, 2469–2473 (2004).
Franco, M., Roswall, P., Cortez, E., Hanahan, D. & Pietras, K. Pericytes promote endothelial cell survival through induction of autocrine VEGF-A signaling and Bcl-w expression. Blood 118, 2906–2917 (2011).
Gonul, E. et al. Early pericyte response to brain hypoxia in cats: an ultrastructural study. Microvasc. Res. 64, 116–119 (2002).
Dore-Duffy, P., Wang, X., Mehedi, A., Kreipke, C.W. & Rafols, J.A. Differential expression of capillary VEGF isoforms following traumatic brain injury. Neurol. Res. 29, 395–403 (2007).
Al Ahmad, A., Gassmann, M. & Ogunshola, O.O. Maintaining blood-brain barrier integrity: pericytes perform better than astrocytes during prolonged oxygen deprivation. J. Cell. Physiol. 218, 612–622 (2009).
Engelhardt, S., Patkar, S. & Ogunshola, O.O. Cell-specific blood-brain barrier regulation in health and disease: a focus on hypoxia. Br. J. Pharmacol. 171, 1210–1230 (2014).
Kim, K.J. et al. Inhibition of vascular endothelial growth factor-induced angiogenesis suppresses tumour growth in vivo. Nature 362, 841–844 (1993).
Kickingereder, P. et al. MR perfusion-derived hemodynamic parametric response mapping of bevacizumab efficacy in recurrent glioblastoma. Radiology 279, 542–552 (2016).
Greenberg, J.I. et al. A role for VEGF as a negative regulator of pericyte function and vessel maturation. Nature 456, 809–813 (2008).
Lu, K.V. et al. VEGF inhibits tumor cell invasion and mesenchymal transition through a MET/VEGFR2 complex. Cancer Cell 22, 21–35 (2012).
Yuan, H.T., Khankin, E.V., Karumanchi, S.A. & Parikh, S.M. Angiopoietin 2 is a partial agonist/antagonist of Tie2 signaling in the endothelium. Mol. Cell. Biol. 29, 2011–2022 (2009).
Felcht, M. et al. Angiopoietin-2 differentially regulates angiogenesis through TIE2 and integrin signaling. J. Clin. Invest. 122, 1991–2005 (2012).
Suri, C. et al. Requisite role of angiopoietin-1, a ligand for the TIE2 receptor, during embryonic angiogenesis. Cell 87, 1171–1180 (1996).
Benest, A.V. et al. Angiopoietin-2 is critical for cytokine-induced vascular leakage. PLoS One 8, e70459 (2013).
Uemura, A. et al. Recombinant angiopoietin-1 restores higher-order architecture of growing blood vessels in mice in the absence of mural cells. J. Clin. Invest. 110, 1619–1628 (2002).
Feng, Y. et al. Impaired pericyte recruitment and abnormal retinal angiogenesis as a result of angiopoietin-2 overexpression. Thromb. Haemost. 97, 99–108 (2007).
Cui, X. et al. Angiopoietin/Tie2 pathway mediates type 2 diabetes induced vascular damage after cerebral stroke. Neurobiol. Dis. 43, 285–292 (2011).
Zhang, L. et al. Tumor-derived vascular endothelial growth factor up-regulates angiopoietin-2 in host endothelium and destabilizes host vasculature, supporting angiogenesis in ovarian cancer. Cancer Res. 63, 3403–3412 (2003).
Nguyen, L.N. et al. Mfsd2a is a transporter for the essential omega-3 fatty acid docosahexaenoic acid. Nature 509, 503–506 (2014).
Ben-Zvi, A. et al. Mfsd2a is critical for the formation and function of the blood-brain barrier. Nature 509, 507–511 (2014).
Alakbarzade, V. et al. A partially inactivating mutation in the sodium-dependent lysophosphatidylcholine transporter MFSD2A causes a non-lethal microcephaly syndrome. Nat. Genet. 47, 814–817 (2015).
Guemez-Gamboa, A. et al. Inactivating mutations in MFSD2A, required for omega-3 fatty acid transport in brain, cause a lethal microcephaly syndrome. Nat. Genet. 47, 809–813 (2015).
Augustin, H.G. & Reiss, Y. EphB receptors and ephrinB ligands: regulators of vascular assembly and homeostasis. Cell Tissue Res. 314, 25–31 (2003).
Salvucci, O. et al. EphrinB reverse signaling contributes to endothelial and mural cell assembly into vascular structures. Blood 114, 1707–1716 (2009).
Foo, S.S. et al. Ephrin-B2 controls cell motility and adhesion during blood-vessel-wall assembly. Cell 124, 161–173 (2006).
Gale, N.W. et al. Ephrin-B2 selectively marks arterial vessels and neovascularization sites in the adult, with expression in both endothelial and smooth-muscle cells. Dev. Biol. 230, 151–160 (2001).
Erber, R. et al. EphB4 controls blood vascular morphogenesis during postnatal angiogenesis. EMBO J. 25, 628–641 (2006).
Garmy-Susini, B. et al. Integrin alpha4beta1-VCAM-1-mediated adhesion between endothelial and mural cells is required for blood vessel maturation. J. Clin. Invest. 115, 1542–1551 (2005).
Gerhardt, H., Wolburg, H. & Redies, C. N-cadherin mediates pericytic-endothelial interaction during brain angiogenesis in the chicken. Dev. Dyn. 218, 472–479 (2000).
Tillet, E. et al. N-cadherin deficiency impairs pericyte recruitment, and not endothelial differentiation or sprouting, in embryonic stem cell-derived angiogenesis. Exp. Cell Res. 310, 392–400 (2005).
Christian, S. et al. Endosialin (Tem1) is a marker of tumor-associated myofibroblasts and tumor vessel-associated mural cells. Am. J. Pathol. 172, 486–494 (2008).
Simonavicius, N. et al. Endosialin (CD248) is a marker of tumor-associated pericytes in high-grade glioma. Mod. Pathol. 21, 308–315 (2008).
MacFadyen, J., Savage, K., Wienke, D. & Isacke, C.M. Endosialin is expressed on stromal fibroblasts and CNS pericytes in mouse embryos and is downregulated during development. Gene Expr. Patterns 7, 363–369 (2007).
Hultman, K., Strickland, S. & Norris, E.H. The APOE ɛ4/ɛ4 genotype potentiates vascular fibrin(ogen) deposition in amyloid-laden vessels in the brains of Alzheimer's disease patients. J. Cereb. Blood Flow Metab. 33, 1251–1258 (2013).
Nishitsuji, K., Hosono, T., Nakamura, T., Bu, G. & Michikawa, M. Apolipoprotein E regulates the integrity of tight junctions in an isoform-dependent manner in an in vitro blood-brain barrier model. J. Biol. Chem. 286, 17536–17542 (2011).
Alata, W., Ye, Y., St-Amour, I., Vandal, M. & Calon, F. Human apolipoprotein E ɛ4 expression impairs cerebral vascularization and blood-brain barrier function in mice. J. Cereb. Blood Flow Metab. 35, 86–94 (2015).
Takano, T. et al. Astrocyte-mediated control of cerebral blood flow. Nat. Neurosci. 9, 260–267 (2006).
Gebremedhin, D. et al. Production of 20-HETE and its role in autoregulation of cerebral blood flow. Circ. Res. 87, 60–65 (2000).
Kamouchi, M. et al. Calcium influx pathways in rat CNS pericytes. Brain Res. Mol. Brain Res. 126, 114–120 (2004).
Sakagami, K., Kawamura, H., Wu, D.M. & Puro, D.G. Nitric oxide/cGMP-induced inhibition of calcium and chloride currents in retinal pericytes. Microvasc. Res. 62, 196–203 (2001).
Nakamura, K. et al. Amiloride inhibits hydrogen peroxide-induced Ca2+ responses in human CNS pericytes. Microvasc. Res. 77, 327–334 (2009).
Mufti, R.E. et al. Intravascular pressure augments cerebral arterial constriction by inducing voltage-insensitive Ca2+ waves. J. Physiol. (Lond.) 588, 3983–4005 (2010).
Zeisel, A. et al. Brain structure. Cell types in the mouse cortex and hippocampus revealed by single-cell RNA-seq. Science 347, 1138–1142 (2015).
Hamel, E. Cholinergic modulation of the cortical microvascular bed. Prog. Brain Res. 145, 171–178 (2004).
Blinder, P. et al. The cortical angiome: an interconnected vascular network with noncolumnar patterns of blood flow. Nat. Neurosci. 16, 889–897 (2013).
Lovick, T.A., Brown, L.A. & Key, B.J. Neurovascular relationships in hippocampal slices: physiological and anatomical studies of mechanisms underlying flow-metabolism coupling in intraparenchymal microvessels. Neuroscience 92, 47–60 (1999).
Shimizu, F. et al. Pericyte-derived glial cell line-derived neurotrophic factor increase the expression of claudin-5 in the blood-brain barrier and the blood-nerve barrier. Neurochem. Res. 37, 401–409 (2012).
Takahashi, H. et al. Brain pericyte-derived soluble factors enhance insulin sensitivity in GT1-7 hypothalamic neurons. Biochem. Biophys. Res. Commun. 457, 532–537 (2015).
Iliff, J.J. et al. A paravascular pathway facilitates CSF flow through the brain parenchyma and the clearance of interstitial solutes, including amyloid β. Sci. Transl. Med. 4, 147ra111 (2012).
Hawkes, C.A. et al. Perivascular drainage of solutes is impaired in the ageing mouse brain and in the presence of cerebral amyloid angiopathy. Acta Neuropathol. 121, 431–443 (2011).
Helbig, H. et al. Membrane potentials in retinal capillary pericytes: excitability and effect of vasoactive substances. Invest. Ophthalmol. Vis. Sci. 33, 2105–2112 (1992).
Li, Q. & Puro, D.G. Adenosine activates ATP-sensitive K(+) currents in pericytes of rat retinal microvessels: role of A1 and A2a receptors. Brain Res. 907, 93–99 (2001).
Wu, D.M., Kawamura, H., Li, Q. & Puro, D.G. Dopamine activates ATP-sensitive K+ currents in rat retinal pericytes. Vis. Neurosci. 18, 935–940 (2001).
Alcendor, D.J. et al. Neurovascular unit on a chip: implications for translational applications. Stem Cell Res. Ther. 4 (suppl. 1), S18 (2013).
Kleinstreuer, N. et al. A computational model predicting disruption of blood vessel development. PLoS Comput. Biol. 9, e1002996 (2013).
Ruck, T., Bittner, S. & Meuth, S.G. Blood-brain barrier modeling: challenges and perspectives. Neural Regen. Res. 10, 889–891 (2015).
Ayyadurai, V.A.S. & Dewey, C.F. CytoSolve: a scalable computational method for dynamic integration of multiple molecular pathway models. Cell. Mol. Bioeng. 4, 28–45 (2011).
Acknowledgements
B.V.Z. is supported by the National Institutes of Health grants R01AG023084, R01NS090904, R01NS034467 and R01AG039452 and the Cure for Alzheimer's Fund.
Author information
Authors and Affiliations
Ethics declarations
Competing interests
S.A. is employed by CytoSolve, Inc. which developed a software-based computational platform for scalable integration of molecular models to offer a systems biology approach to pathway analysis.
Integrated supplementary information
Supplementary Figure 1 Signal transduction pathways of endothelial cells: expanded details of ‘NVU cells’ layer in the NVU integrated pathway model.
The numbered boxes partition the cell’s downstream molecular events and the arrows between boxes illustrate interactions amongst pathways. Additional signal transduction events can be modularly incorporated into this model, as indicated in box 12. Multiple signal transduction events can promote a given function (denoted in yellow box). Specific downstream signaling mechanisms and resulting transcriptional gene expression/inhibition in endothelial cells can directly promote or inhibit signaling with pericytes (see ‘interactive signaling’ in Figure 6) that, when awry, can contribute to dysfunction in major neurological disorders (see ‘Disorders’ in Figure 6).
Supplementary Figure 2 Signal transduction pathways of pericytes: expanded details of ‘NVU cells’ layer in the NVU integrated pathway model.
The numbered boxes partition the cell’s downstream molecular events and the arrows between boxes illustrate interactions amongst pathways. Additional signal transduction events can be modularly incorporated into this model, as indicated in box 13. Multiple signal transduction events can promote a given function (denoted in yellow box). Specific downstream signaling mechanisms and resulting transcriptional gene expression/inhibition in endothelial cells can directly promote or inhibit signaling with endothelial cells or astrocytes (see ‘interactive signaling’ in Figure 6) that, when awry, can contribute to dysfunction in major neurological disorders (see ‘Disorders’ in Figure 6).
Supplementary Figure 3 Signal transduction pathways of astrocytes: expanded details of ‘NVU cells’ layer in the NVU integrated pathway model.
The numbered boxes partition the cell’s downstream molecular events and the arrows between boxes illustrate interactions amongst pathways. Additional signal transduction events can be modularly incorporated into this model, as indicated in box 2. Specific downstream signaling mechanisms and resulting transcriptional gene expression/inhibition in endothelial cells can directly promote or inhibit signaling with pericytes (see ‘interactive signaling’ in Figure 6) that, when awry, can contribute to dysfunction in major neurological disorders (see ‘Disorders’ in Figure 6).
Supplementary information
Supplementary Text and Figures
Supplementary Figures 1-3 (PDF 651 kb)
Rights and permissions
About this article
Cite this article
Sweeney, M., Ayyadurai, S. & Zlokovic, B. Pericytes of the neurovascular unit: key functions and signaling pathways. Nat Neurosci 19, 771–783 (2016). https://doi.org/10.1038/nn.4288
Received:
Accepted:
Published:
Issue Date:
DOI: https://doi.org/10.1038/nn.4288
This article is cited by
-
Effect of breast milk intake volume on early behavioral neurodevelopment of extremely preterm infants
International Breastfeeding Journal (2024)
-
Microvascular destabilization and intricated network of the cytokines in diabetic retinopathy: from the perspective of cellular and molecular components
Cell & Bioscience (2024)
-
Understanding the link between neurotropic viruses, BBB permeability, and MS pathogenesis
Journal of NeuroVirology (2024)
-
Brain Pathology in COVID-19: Clinical Manifestations and Potential Mechanisms
Neuroscience Bulletin (2024)
-
Loss of Direct Vascular Contact to Astrocytes in the Hippocampus as an Initial Event in Alzheimer’s Disease. Evidence from Patients, In Vivo and In Vitro Experimental Models
Molecular Neurobiology (2024)