We thank Laura Denti, Valentina Senatore and the staff of the Biological Resources Unit at the UCL Institute of Ophthalmology for help with mouse husbandry and Camille Charoy for technical support. This work was supported by a Medical Research Council grant (MR/N011511/1) to C. Ruhrberg and a British Heart Foundation PhD studentship to J.T. Brash (FS/13/59/30649).

All animal work was carried out following UK Home Office and institutional Animal Welfare and Ethical Review Body (AWERB) guidelines.
1. Mouse Preparation
NOTE: Perform experiments on adult mice of at least 8 weeks of age, up to 6 months of age. In order to demonstrate technical reproducibility and consistent timing for each step of this procedure between different animals, use a minimum of 2 and maximum of 6 mice for each experimental session. To evaluate the effect of a mutation on a permeability-inducing substance in genetically modified mice, ideally, use 2 mutant mice and 2 littermate controls per experiments.
<ol>
	<li>24 h prior to stimulating vascular hyperpermeability, anesthetize mice using a suitable inhalation anesthetic such as isoflurane. Use 3% isoflurane for anesthesia induction until the righting reflex is lost and the mouse is unresponsive to external stimuli. Use 1.5% isoflurane for anesthesia maintenance (ensure that the mouse has constant respiratory rates). Under anesthesia, carefully shave both flanks of each mouse with an electrical shaver, avoiding injuries to the skin. 
	NOTE: Anesthesia is used to avoid causing stress to the animal and to minimize movement during shaving, which may result in skin damage.</li>
	<li>Return the shaved mouse to its home cage. For male mice, place each male into an individual cage after anesthesia recovery to prevent fighting and, therefore, damaging the skin. For female mice, return them in a group to their home cage. 
	NOTE: If a fighting behavior is observed among male mice in the cage, before the procedure, separate them into individual cages for 3 days before the experiment to allow potential skin damage to heal.</li>
	<li>Monitor the mice until they recover consciousness (usually within a few seconds) and move around the cage (usually within 1 min).</li>
</ol>
2. Intravenous Injection of Evans Blue Dye
<ol>
	<li>In a laminar flow cabinet, prepare separate sterile solutions of the histamine inhibitor pyrilamine maleate (4 &#181;g/&#181;L in 0.9% saline) and of Evans blue dye (1% w/v in 0.9% saline). Sterilize by passing the solutions through a 22 &#181;m filter.</li>
	<li>Use a sterile 1 mL syringe with a 30 G needle to intraperitoneally inject each mouse with 10 &#181;L pyrilamine maleate solution/gram of body weight (Figure 1A). To perform the injection, first, scruff the mouse and then tilt it so that the head is directed towards the ground and the abdomen is directed upwards. Inject in the lower quadrants of the abdomen away from the midline to avoid hitting the bladder. 
	NOTE: The weight of mice between 8 weeks and 6 months of age usually ranges between 15 and 30 g. Pyrilamine maleate will inhibit the release of endogenous histamine, which would otherwise promote vascular leakage independently of the agent to be tested.</li>
	<li>Place the mouse in a 37 &#176;C heat chamber for 10 min to promote vasodilation. Alternatively, use a suitable heat lamp focused on the tail to promote vasodilation if the use of a heat lamp is permitted by the local ethical guidelines.</li>
	<li>Move one mouse at a time to a mouse restrainer and rub the tail with 70% ethanol to clean the injection area and further promote vasodilation.</li>
	<li>Use a sterile 1 mL syringe with a 30G needle to administer 100 &#181;L Evans blue dye intravenously through the tail vein (Figure 1B). Immediately apply pressure to the injection site by holding the tail between a finger and the thumb to prevent bleeding. 
	NOTE: Visualization of the tail vein can be improved by directing the lamplight to the injection area. Further detail on performing intravenous injections into the mouse tail vein can be found in a published protocol18.</li>
	<li>Allow the dye to circulate for 30 min.</li>
</ol>
3. Stimulate Vascular Hyperpermeability
<ol>
	<li>Using sterile solutions in a laminar flow cabinet, dilute the permeability-inducing agent of interest to a concentration that allows the final dose to be delivered in a volume of 20 &#181;L. 
	NOTE: In the example experiment shown in Figure 1-Figure 2, VEGFA is used to stimulate vascular hyperpermeability at a concentration of 2.5 ng/&#181;L in PBS, yielding a total dose of 50 ng, and PBS is used as a vehicle control.</li>
	<li>Load the permeability-inducing agent of interest and the vehicle control into 2 separate sterile 300 &#181;L syringes with a 31 G needle. Load sufficient solution to inject each mouse with 20 &#181;L of the solution in triplicate (i.e. prepare 60 &#181;L of agent and vehicle per mouse, plus additional volume to account for the needle&#39;s dead volume).</li>
	<li>Anesthetize the first mouse to be tested with isoflurane (3% for anesthesia induction until righting reflex is lost and the mouse is unresponsive to external stimuli, and 1.5% for anesthesia maintenance, making sure that the mouse has constant respiratory rates).</li>
	<li>Intradermally inject 20 &#181;L of the permeability-promoting agent into the flank of the mouse (Figure 1C). Ensure that the needle is at an angle of 15&#176; to the skin. Check for the formation of a raised bubble within the skin which indicates a successful injection. Repeat the intradermal injection at 2 additional sites, a least 1 cm apart.</li>
	<li>Turn the mouse to expose the 2nd flank and repeat triplicate injections with the control vehicle solution. Record on paper the position of each injection site to facilitate their identification for subsequent collection of skin samples. 
	NOTE: Handle the mouse skin with caution at this stage; for example, avoid pinching the skin when performing intradermal injections.</li>
	<li>Return the injected mouse to its home cage and monitor the mouse until it recovers consciousness (usually within a few seconds) and moves around the cage.</li>
	<li>Whilst the first mouse recovers, immediately repeat steps 3.3 and 3.5 with the second mouse, and so on (up to 6 mice maximally per session). Keep a record of the time each mouse was injected to adjust the time at which to proceed to the subsequent step.</li>
</ol>
4. Quantification of Accumulated Evans Blue Within the Dermis
<ol>
	<li>Cull each mouse by cervical dislocation 20 min after it has received the intradermal injections, observing the same order in which the mice were injected. 
	NOTE: The duration of vascular leakage may vary according to the permeability-inducing agent used, and, therefore, the time between intradermal injection and culling may need optimizing.</li>
	<li>Place each culled mouse on its back and pin its feet onto a cork board wrapped with a clean tissue (Figure 1D).</li>
	<li>Using blunt scissors, make a vertical incision of approximately 3 - 4&#160;cm from the lower abdomen up to the chest of the dead mouse. With forceps and a scalpel, tease away the skin from both flanks to reveal the inner side of the dermis and sites of Evans blue accumulation (Figure 1E). Pin down the loose skin and remove fat from regions around the leakage site with a scalpel. If required, take a representative photo to demonstrate the magnitude of Evans blue leakage into the skin.</li>
	<li>Using forceps and a scalpel, excise skin regions comprising the leaked Evans blue dye for each site injected with the permeability-inducing agent or vehicle. 
	NOTE: Take care to excise similarly sized regions of the skin to make sure that, at the subsequent Step 4.7, a similar portion of the formamide volume will be adsorbed by each skin sample, allowing the extracted dye to be diluted in a similar volume of remaining formamide. The injection map recorded in step 3.5 will help define the area to be excised.</li>
	<li>Place each sample into a 1.5 mL tube and labeled it accordingly, making sure each sample rests on the bottom of the tube. Store the samples at - 20 &#176;C until further use. If processing immediately, follow the steps below.</li>
	<li>Dry the skin samples overnight by placing open tubes in an oven or into the well of a heating block at 55 &#176;C.</li>
	<li>To extract Evans blue dye, add 250 &#181;L of deionized formamide to the samples in a fume hood, close the tubes. Make sure the skin samples are all covered by the formamide and incubate overnight in an oven or a heating block at 55 &#176;C.</li>
	<li>Centrifuge samples in a benchtop centrifuge at maximal speed (&#62;10,000 x g) for 40 min.</li>
	<li>In a fume hood, transfer 100 &#181;L of the dye-containing supernatant from each sample into a separate well of a transparent, flat bottom 96-well plate (Figure 2A).</li>
	<li>Measure peak Evans blue absorbance at 620 nm with a reference reading of 740 nm on a spectrophotometer. 
	NOTE: 620 nm is the peak of Evans blue absorbance, whilst 740 nm is not absorbed by Evans blue and acts as a reference wavelength.</li>
	<li>Average the absorbance readings of triplicate injections of the same agent or vehicle for each mouse to account for technical variability (Figure 2B).</li>
	<li>Calculate the fold difference of readings from permeability-inducing agent versus vehicle control (Figure 2C).</li>
</ol>

<ol>
	<li>Nagy, J. A., Benjamin, L., Zeng, H. Y., Dvorak, A. M., Dvorak, H. F. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Vascular+permeability,+vascular+hyperpermeability+and+angiogenesis.">Vascular permeability, vascular hyperpermeability and angiogenesis.</a> Angiogenesis. 11, 109-119 (2008).</li><li>Engelhardt, B. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Development+of+the+blood-brain+barrier.">Development of the blood-brain barrier.</a> Cell and Tissue Research. 314, 119-129 (2003).</li><li>Ruhrberg, C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Growing+and+shaping+the+vascular+tree:+multiple+roles+for+VEGF.">Growing and shaping the vascular tree: multiple roles for VEGF.</a> Bioessays. 25, 1052-1060 (2003).</li><li>Risau, W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Differentiation+of+Endothelium.">Differentiation of Endothelium.</a> FASEB Journal. 9, 926-933 (1995).</li><li>Strbian, D., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=The+blood-brain+barrier+is+continuously+open+for+several+weeks+following+transient+focal+cerebral+ischemia.">The blood-brain barrier is continuously open for several weeks following transient focal cerebral ischemia.</a> Neuroscience. 153, 175-181 (2008).</li><li>Weis, S. M., Cheresh, D. A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Pathophysiological+consequences+of+VEGF-induced+vascular+permeability.">Pathophysiological consequences of VEGF-induced vascular permeability.</a> Nature. 437, 497-504 (2005).</li><li>Campochiaro, P. A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Molecular+pathogenesis+of+retinal+and+choroidal+vascular+diseases.">Molecular pathogenesis of retinal and choroidal vascular diseases.</a> Progress in Retinal and Eye Research. 49, 67-81 (2015).</li><li>Aman, J., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Effective+Treatment+of+Edema+and+Endothelial+Barrier+Dysfunction+with+Imatinib.">Effective Treatment of Edema and Endothelial Barrier Dysfunction with Imatinib.</a> Circulation. , 126 (2012).</li><li>Claesson-Welsh, L. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Vascular+permeability-the+essentials.">Vascular permeability-the essentials.</a> Upsala J Med Sci. 120, 135-143 (2015).</li><li>Schulte, D., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Stabilizing+the+VE-cadherin-catenin+complex+blocks+leukocyte+extravasation+and+vascular+permeability.">Stabilizing the VE-cadherin-catenin complex blocks leukocyte extravasation and vascular permeability.</a> Embo Journal. 30, 4157-4170 (2011).</li><li>Heinolainen, K., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=VEGFR3+Modulates+Vascular+Permeability+by+Controlling+VEGF/VEGFR2+Signaling.">VEGFR3 Modulates Vascular Permeability by Controlling VEGF/VEGFR2 Signaling.</a> Circulation Research. 120, (2017).</li><li>Eliceiri, B. P., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Selective+requirement+for+Src+kinases+during+VEGF-induced+angiogenesis+and+vascular+permeability.">Selective requirement for Src kinases during VEGF-induced angiogenesis and vascular permeability.</a> Molecular Cell. 4, 915-924 (1999).</li><li>Sun, Z. Y., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=VEGFR2+induces+c-Src+signaling+and+vascular+permeability+in+vivo+via+the+adaptor+protein+TSAd.">VEGFR2 induces c-Src signaling and vascular permeability in vivo via the adaptor protein TSAd.</a> Journal of Experimental Medicine. 209, 1363-1377 (2012).</li><li>Fantin, A., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=VEGF165-induced+vascular+permeability+requires+NRP1+for+ABL-mediated+SRC+family+kinase+activation.">VEGF165-induced vascular permeability requires NRP1 for ABL-mediated SRC family kinase activation.</a> Journal of Experimental Medicine. 214, 1049-1064 (2017).</li><li>Li, X. J., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=VEGFR2+pY949+signalling+regulates+adherens+junction+integrity+and+metastatic+spread.">VEGFR2 pY949 signalling regulates adherens junction integrity and metastatic spread.</a> Nat Commun. 7, (2016).</li><li>Senger, D. R., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Tumor+cells+secrete+a+vascular+permeability+factor+that+promotes+accumulation+of+ascites+fluid.">Tumor cells secrete a vascular permeability factor that promotes accumulation of ascites fluid.</a> Science. 219, 983-985 (1983).</li><li>Miles, A. A., Miles, E. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Vascular+Reactions+to+Histamine,+Histamine-Liberator+and+Leukotaxine+in+the+Skin+of+Guinea-Pigs.">Vascular Reactions to Histamine, Histamine-Liberator and Leukotaxine in the Skin of Guinea-Pigs.</a> J Physiol-London. 118, 228-257 (1952).</li><li>Radu, M., Chernoff, J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=An+in+vivo+Assay+to+Test+Blood+Vessel+Permeability.">An in vivo Assay to Test Blood Vessel Permeability.</a> Jove-J Vis Exp. , e50062 (2013).</li><li>Roth, L., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Neuropilin-1+mediates+vascular+permeability+independently+of+vascular+endothelial+growth+factor+receptor-2+activation.">Neuropilin-1 mediates vascular permeability independently of vascular endothelial growth factor receptor-2 activation.</a> Sci Signal. 9, (2016).</li><li>Acevedo, L. M., Barillas, S., Weis, S. M., Gothert, J. R., Cheresh, D. A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Semaphorin+3A+suppresses+VEGF-mediated+angiogenesis+yet+acts+as+a+vascular+permeability+factor.">Semaphorin 3A suppresses VEGF-mediated angiogenesis yet acts as a vascular permeability factor.</a> Blood. 111, 2674-2680 (2008).</li><li>Teesalu, T., Sugahara, K. N., Kotamraju, V. R., Ruoslahti, E. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=C-end+rule+peptides+mediate+neuropilin-1-dependent+cell,+vascular,+and+tissue+penetration.">C-end rule peptides mediate neuropilin-1-dependent cell, vascular, and tissue penetration.</a> P Natl Acad Sci USA. 106, 16157-16162 (2009).</li><li>Ho, V. C., Duan, L. J., Cronin, C., Liang, B. T., Fong, G. H. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Elevated+Vascular+Endothelial+Growth+Factor+Receptor-2+Abundance+Contributes+to+Increased+Angiogenesis+in+Vascular+Endothelial+Growth+Factor+Receptor-1-Deficient+Mice.">Elevated Vascular Endothelial Growth Factor Receptor-2 Abundance Contributes to Increased Angiogenesis in Vascular Endothelial Growth Factor Receptor-1-Deficient Mice.</a> Circulation. 126, (2012).</li><li>Chislock, E. M., Pendergast, A. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Abl+Family+Kinases+Regulate+Endothelial+Barrier+Function+In+Vitro+and+in+Mice.">Abl Family Kinases Regulate Endothelial Barrier Function In Vitro and in Mice.</a> PLoS ONE. 8, e85231 (2013).</li><li>Busch, C. J., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Effects+of+ketamine+on+hypoxic+pulmonary+vasoconstriction+in+the+isolated+perfused+lungs+of+endotoxaemic+mice.">Effects of ketamine on hypoxic pulmonary vasoconstriction in the isolated perfused lungs of endotoxaemic mice.</a> Eur J Anaesth. 27, 61-66 (2010).</li><li>Sinclair, M. D. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+review+of+the+physiological+effects+of+alpha2-agonists+related+to+the+clinical+use+of+medetomidine+in+small+animal+practice.">A review of the physiological effects of alpha2-agonists related to the clinical use of medetomidine in small animal practice.</a> Can Vet J. 44, 885-897 (2003).</li></ol>

The authors have no conflicting interests to declare.

Since its first description in 195217, the Miles assay has provided researchers with a relatively quick, simple, and reliable method for studying the molecular mechanisms of vascular hyperpermeability. For example, the Miles assay has been used to test the ability and/or potency of different agents to induce hyperpermeability19,20,21 or to test the efficacy of hyperpermeability blocking agents8,22,23. As another example, agents that induce vascular permeability have been tested in genetically modified mice and their littermate controls to determine the requirements of specific receptors and signal transducing proteins for ligand-induced hyperpermeability responses10,11,12,13,14,15,20,23. Several modified versions of the Miles assay have since been used, for example with respect to the tracer used. Thus, Evans Blue has been substituted in some studies with fluorescence-labeled dextrans of different sizes or microspheres11,13.
The main advantage of the Miles assay over other assays for investigating vascular hyperpermeability mechanisms is that it is comparatively easy to perform and does not require expensive equipment. Furthermore, as an in vivo technique, this assay models&#160;vascular leakage in the context of intact blood vessels, as opposed to measuring leakage through in vitro assays such as trans well flux assays or trans endothelial electrical resistance (TEER) assays, which focus, solely, on the endothelial monolayer. The alternative in vivo assays of vascular hyperpermeability may differ from the Miles assay described here by utilizing a different delivery route for the hyperpermeability-inducing agent or by analyzing vascular leakage at different sites, for example by systemic delivery of an agent via the tail vein followed by vascular leakage examination in the lungs or the trachea11,13,15. One limitation of the Miles assay is that the intradermal injection of certain agents may, in principle, also influence blood pressure and flow in addition to endothelial barrier disruption and, therefore, influence vascular permeability also indirectly. Nevertheless, this assay has recently been shown to measure vascular permeability induced by VEGF-A independently of effects on systemic blood pressure15. Another limitation of the Miles assay is that vascular beds in different tissues may respond differently to permeability-promoting agents, and results obtained with a Miles assay in the skin may, therefore, not be representative, for example, of what occurs in the lung or brain.
Animal&#39;s age and weight may influence the leakage observed in the Miles assay. To minimize the effect of these variables, researchers should use littermates or similarly sized and aged mice as controls. When assessing mouse mutants for a particular gene of interest, mice should be generated through a heterozygous versus heterozygous breeding strategy and wildtype littermates used as controls. Moreover, it is advisable to use quickly reversible gas anesthetics, such as isoflurane, to avoid vasoconstriction, which has been described for some anesthetic drug administered via parenteral injections24,25. The injection of Evans blue dye into the mouse lateral tail vein is a critical step in this protocol and can greatly influence the quality of the experiment and data. Thus, researchers must be competent in performing tail vein injections and will likely need prior experience or practice before beginning the Miles assay experiment. Alternatively, researchers could use other intravenous routes to deliver Evans blue, such as retro-orbital injection if they are experienced with it. Intradermal injection of permeability-promoting solutions can cause agent-independent damage to the skin. Therefore, intradermal injections should not exceed 20 &#181;l in volume, should always be carried out in the presence of the histamine inhibitor and normalized to vehicle control injections.
The Miles assay has been used by many researchers to evaluate components of the VEGF-A signaling pathway, for example, because VEGF-A-induced vascular permeability causes ascites in cancer patients16 and vision-impairing edema in several neovascular eye disease7. Thus, we and others have used the Miles assay to compare VEGF-A induced vascular leakage in mice that have been genetically modified to lack specific components of the VEGF-A signaling cascade12,13,14,15,20,23. Our recent study using this approach revealed that the main pathological VEGF-A isoform, VEGF165, signals through a complex of VEGFR2 and NRP1, in which the NRP1 cytoplasmic domain promotes the ABL kinase-mediated activation of SRC family kinases to evoke a hyperpermeability response14. VEGFA also promotes blood vessel growth and could, therefore, be used therapeutically to restore blood flow to ischemic tissues if its hyperpermeability activities could be specifically inhibited. Research elucidating the molecular mechanism that steers VEGF-A responses of vascular endothelial cells towards vascular hyperpermeability might, therefore, identify pathways that can be selectively manipulated to inhibit pathological VEGF-A induced edema in diseases, such as cancer or ischemic eye disease. The Miles assay will undoubtedly continue to be a helpful method to underpin these and many other types of functional studies to elucidate molecular regulators and effectors of vascular hyperpermeability.

The primary function of the cardiovascular system is to enable the transfer of gases, nutrients, and waste products between the circulation and tissues in all organs. Blood vessels have organ-specific levels of basal permeability to permit such exchanges1. For instance, blood vessels in the kidney are highly permeable, whilst the blood brain barrier forms a tight, highly impenetrable interface2,3,4. The endothelial cells that form the inner lining of blood vessels provide a physical barrier between the circulation and underlying tissues and regulate vascular permeability in an organ-specific manner. However, certain stimuli cause a partial breakdown of the endothelial barrier to increase the fluid extravasation from the circulation into the interstitium above the basal levels1. Such hyperpermeability is observed, for example, at sites of tissue trauma, in inflammation, in tumors, during sepsis, in eyes with neovascular disease or in the brain and heart, when tissue ischemia occurs due to a stroke or myocardial infarction, respectively5,6,7,8. When chronically elevated, hyperpermeability leads to edema, which in turn causes tissue damage, such as loss of vision in eye disease9. Thus, modeling the vascular hyperpermeability response is desirable for understanding the mechanisms that increase endothelial permeability and to test the efficacy of agents designed to inhibit this.
The Miles assay is a well-established, commonly used and relatively simple technique that measures vascular leakage in vivo as a surrogate measurement of vascular hyperpermeability. Even though it does not take into account compounding factors that may increase vascular leakage independently of endothelial barrier regulation, such as blood pressure or blood flow, the Miles assay is generally thought to provide a reliable method to evaluate the permeability-modulating activity of substances and identify the signaling mediators that promote their activity. Accordingly, the Miles assay has been integral to numerous studies that have identified mediators of vascular hyperpermeability and their mechanisms of action10,11,12,13,14,15, such as the vascular endothelial growth factor VEGF-A that was originally identified as the vascular permeability factor VPF16.
Originally developed by Miles and Miles to study vascular permeability in guinea pigs17, their assay was subsequently adapted to using mice, which are now the model organism of choice to elucidate molecular mechanisms of vascular permeability regulation due to their exquisite suitability to genetic manipulation. Briefly, Evans blue dye is intravenously injected into adult mice and allowed to circulate for 30 minutes (Figure 1). Permeability-inducing agents versus vehicle control are then intradermally injected in multiple sites on opposing flanks of the mouse to induce vascular leak (Figure 1). Consequently, albumin-bound Evans blue dye extravasates and accumulates in the dermis (Figure 1). After humanely culling the mouse, Evans blue is extracted from the dermis and the level of vascular leak calculated as a ratio of test substance- to vehicle-induced optical density (Figure 2).

<table><tbody><tr><td>Pyrilamine maleate salt</td><td>Sigma-Aldrich</td><td>P5514-5G</td><td>Resuspend in PBS</td></tr><tr><td>Deionised Formamide</td><td>Sigma-Aldrich</td><td>S4117</td><td>Use in fume cupboard</td></tr><tr><td>Microlance Needles 30g x 0.5&quot;</td><td>BD&amp;nbsp;</td><td>305106</td><td></td></tr><tr><td>Sterile Plastipak 1ml Luer</td><td>BD&amp;nbsp;</td><td>309659</td><td></td></tr><tr><td>Sterile MicroFine syriinges 0.3 ml - 8 mm - 30G&amp;nbsp;</td><td>BD&amp;nbsp;</td><td>324826</td><td></td></tr><tr><td>Evans blue</td><td>Sigma Aldrich</td><td>E2129</td><td></td></tr><tr><td>Mouse restrainer</td><td></td><td></td><td></td></tr><tr><td>Heat chamber</td><td></td><td></td><td></td></tr><tr><td>Hair clippers</td><td></td><td></td><td></td></tr><tr><td>Isoflurane</td><td>Merial</td><td>ap/drugs/220/96</td><td></td></tr><tr><td>Scalpal&amp;nbsp;</td><td></td><td></td><td></td></tr><tr><td>Blunt scissor</td><td></td><td></td><td></td></tr><tr><td>Forceps</td><td></td><td></td><td></td></tr><tr><td>Eppendorf tubes</td><td></td><td></td><td></td></tr><tr><td>Heatblock</td><td></td><td></td><td></td></tr><tr><td>Cork board</td><td></td><td></td><td></td></tr><tr><td>Benchtop refrigerated centrifuge</td><td></td><td></td><td></td></tr><tr><td>Recombinant Vascular Endothelial Growth Factor 165</td><td>Reliatech</td><td>M30-004</td><td></td></tr></tbody></table>

evaluating vascular hyperpermeability-inducing agents in the skin with the miles assay

The primary function of the vascular endothelium in vertebrate organisms is to serve as a barrier between the blood and each tissue of the body, whereby the permeability of the endothelium to blood cells, plasma macromolecules, and water can be adapted according to the physiological need. In certain diseases, cytokines and growth factors are released that target the endothelial barrier to transiently increase vascular permeability; however, their prolonged presence may cause chronic vascular hyperpermeability and thereby tissue-damaging edema. The Miles assay is an in vivo technique that allows researchers to study vascular hyperpermeability through the proxy measurement of vascular leakage. Here, we provide a detailed protocol on how to perform this procedure in the mouse, which is the most widely used model organism to study mammalian physiology and pathology. The procedure involves the intravenous injection of Evans blue dye to label the circulating albumin followed by multiple intradermal injections of permeability-inducing agents and vehicle control solutions into opposing flanks of the mouse. Consequently, Evans blue dye gradually leaks into the dermis, where it accumulates and can be extracted for quantification as leakage induced by the permeability-inducing agent relative to the vehicle. The Miles assay can be performed in wild type or genetically modified mouse models and may be combined with drug administration to study molecular mechanisms that regulate vascular permeability and identify agents/targets capable of inducing or blocking hyperpermeability.

We used the Miles assay to assess the ability of VEGF-A to induce vascular leak relative to vehicle control (PBS) in wildtype C57/Bl6 mice. Here, we show a representative experiment using wildtype mice stimulated with intradermal injection of 20 &#181;L solution containing 50 ng of VEGF-A in PBS or vehicle PBS only. A clear increase in Evans blue dye leakage in skin samples injected with VEGF-A compared to PBS was apparent in situ (Figure 1E) and after extraction of the dye in formamide (Figure 2A). Quantification of multiple experiments illustrates that 50 ng of VEGF-A significantly induces more Evans blue leakage than PBS alone (Figure 2B), with an average 3-fold increase in vascular leakage compared to vehicle (Figure 2C).
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/57524/57524fig1.jpg" /> 
Figure 1: Induction of vascular leakage in the Miles assay. Schematic representation (top panels) and corresponding images (bottom panels) of the sequential steps when performing the Miles assay in the mouse. (A) Pyrilamine maleate is injected intraperitoneally to prevent the release of endogenous histamine 10 to 30 minutes prior to (B) intravenous injection of 100 &#181;l 1% Evans blue into the tail vein of the mouse. (C) 30 min later, vascular leakage is induced by intradermal injection of the agent (50 ng of VEGF-A; green circles) versus vehicle control (PBS; white circles). (D, E) To access sites of Evans blue accumulation, the mouse is culled 20 minutes after the intradermal injections and the skin of both flanks dissected and pinned down. i.p.: intraperitoneal; i.v.: intravenous; i.d.: intradermal; scale bars, 1 cm. <a href="/files/ftp_upload/57524/57524fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/57524/57524fig2.jpg" /> 
Figure 2: Quantification of vascular leakage in the Miles assay. (A) Evans blue dye is extracted in formamide from skin samples obtained from each intradermal injection in Figure 1 and loaded into a 96-well plate for absorbance reading with a spectrophotometer. (B, C) Graphical representation of the absorbance readings from multiple experiments by plotting either (B) the normalized absorbance values (optical density, OD) of both the permeability-inducing agent (VEGF-A; dark green circles) and vehicle (PBS; grey circles), or (C) the fold change in OD for the agent versus vehicle (error bars: SEM). The absorbance readings of the triplicate PBS and VEGF-A samples shown in (A) are averaged and shown in (B, C) as white or green circles, respectively. <a href="/files/ftp_upload/57524/57524fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Evaluating Vascular Hyperpermeability-inducing Agents in the Skin with the Miles Assay at JoVE.com

Evaluating Vascular Hyperpermeability-inducing Agents in the Skin with the Miles Assay

Here, we present a protocol to measure the vascular leakage induced by intradermal administration of permeability promoting agents into the murine skin. This technique can be used to determine the ability of molecules to promote or inhibit vascular leakage or to study the molecular mechanisms that regulate vascular permeability.

The primary function of the vascular endothelium in vertebrate organisms is to serve as a barrier between the blood and each tissue of the body, whereby ...

evaluating-vascular-hyperpermeability-inducing-agents-skin-with-miles

Research

JoVE Journal

Biology

14.7K Views.  University College London. Here, we present a protocol to measure the vascular leakage induced by intradermal administration of permeability promoting agents into the murine skin. This technique can be used to determine the ability of molecules to promote or inhibit vascular leakage or to study the molecular mechanisms that regulate vascular permeability.

Video: Evaluating Vascular Hyperpermeability-inducing Agents in the Skin with the Miles Assay

Assessment of Endothelial Cell Migration After Exposure to Toxic Chemicals

Exposure to chemical substances (including alkylating chemical warfare agents like sulfur and nitrogen mustards) cause a plethora of clinical symptoms including wound healing disorder. The physiological process of wound healing is highly complex. The formation of granulation tissue is a key step in this process resulting in a preliminary wound closure and providing a network of new capillary blood vessels &#8211; either through vasculogenesis (novel formation) or angiogenesis (sprouting of existing vessels). Both vasculo- and angiogenesis require functional, directed migration of endothelial cells. Thus, investigation of early endothelial cell (EEC) migration is important to understand the pathophysiology of chemical induced wound healing disorders and to potentially identify novel strategies for therapeutic intervention.
We assessed impaired wound healing after alkylating agent exposure and tested potential candidate compounds for treatment. We used a set of techniques outlined in this protocol. A modified Boyden chamber to quantitatively investigate chemokinesis of EEC is described. Moreover, the use of the wound healing assay in combination with track analysis to qualitatively assess migration is illustrated. Finally, we demonstrate the use of the fluorescent dye TMRM for the investigation of mitochondrial membrane potential to identify underlying mechanisms of disturbed cell migration. The following protocol describes basic techniques that have been adapted for the investigation of EEC.

Investigation of early endothelial cell (EEC) migration is important to understand the pathophysiology of certain illnesses and to potentially identify novel strategies for therapeutic intervention. The following protocol describes techniques to assess cell migration that have been adapted for the investigation of EEC.

Exposure to chemical substances (including alkylating chemical warfare agents like sulfur and nitrogen mustards) cause a plethora of clinical symptoms ...

Developmental Biology

Assessing Tumor Microenvironment of Metastasis Doorway-Mediated Vascular Permeability Associated with Cancer Cell Dissemination using Intravital Imaging and Fixed Tissue Analysis

The most common cause of cancer related mortality is metastasis, a process that requires dissemination of cancer cells from the primary tumor to secondary sites. Recently, we established that cancer cell dissemination in primary breast cancer and at metastatic sites in the lung occurs only at doorways called Tumor MicroEnvironment of Metastasis (TMEM). TMEM doorway number is prognostic for distant recurrence of metastatic disease in breast cancer patients. TMEM doorways are composed of a cancer cell which over-expresses the actin regulatory protein Mena in direct contact with a perivascular, proangiogenic macrophage which expresses high levels of TIE2 and VEGF, where both of these cells are tightly bound to a blood vessel endothelial cell. Cancer cells can intravasate through TMEM doorways due to transient vascular permeability orchestrated by the joint activity of the TMEM-associated macrophage and the TMEM-associated Mena-expressing cancer cell. In this manuscript, we describe two methods for assessment of TMEM-mediated transient vascular permeability: intravital imaging and fixed tissue immunofluorescence. Although both methods have their advantages and disadvantages, combining the two may provide the most complete analyses of TMEM-mediated vascular permeability as well as microenvironmental prerequisites for TMEM function. Since the metastatic process in breast cancer, and possibly other types of cancer, involves cancer cell dissemination via TMEM doorways, it is essential to employ well established methods for the analysis of the TMEM doorway activity. The two methods described here provide a comprehensive approach to the analysis of TMEM doorway activity, either in na&#239;ve or pharmacologically treated animals, which is of paramount importance for pre-clinical trials of agents that prevent cancer cell dissemination via TMEM.

We describe two methods for assessing transient vascular permeability associated with tumor microenvironment of metastasis (TMEM) doorway function and cancer cell intravasation using intravenous injection of high-molecular weight (155 kDa) dextran in mice. The methods include intravital imaging in live animals and fixed tissue analysis using immunofluorescence.

The most common cause of cancer related mortality is metastasis, a process that requires dissemination of cancer cells from the primary tumor to secondary ...

Cancer Research

An in vivo Assay to Test Blood Vessel Permeability

This method is based on the intravenous injection of Evans Blue in mice as the test animal model. Evans blue is a dye that binds albumin. Under physiologic conditions the endothelium is impermeable to albumin, so Evans blue bound albumin remains restricted within blood vessels. In pathologic conditions that promote increased vascular permeability endothelial cells partially lose their close contacts and the endothelium becomes permeable to small proteins such as albumin. This condition allows for extravasation of Evans Blue in tissues. A healthy endothelium prevents extravasation of the dye in the neighboring vascularized tissues. Organs with increased permeability will show significantly increased blue coloration compared to organs with intact endothelium. The level of vascular permeability can be assessed by simple visualization or by quantitative measurement of the dye incorporated per milligram of tissue of control versus experimental animal/tissue. Two powerful aspects of this assay are its simplicity and quantitative characteristics. Evans Blue dye can be extracted from tissues by incubating a specific amount of tissue in formamide. Evans Blue absorbance maximum is at 620 nm and absorbance minimum is at 740 nm. By using a standard curve for Evans Blue, optical density measurements can be converted into milligram dye captured per milligram of tissue. Statistical analysis should be used to assess significant differences in vascular permeability.

An in vivo Assay to Test Blood Vessel Permeability

We are presenting an in vivo assay to test blood vessel permeability. This assay is based on intravenous injection of a dye and subsequent visualization of its diffusion into interstitial spaces.

This method is based on the intravenous injection of Evans Blue in mice as the test animal model. Evans blue is a dye that binds albumin. Under ...

Medicine

A Full Skin Defect Model to Evaluate Vascularization of Biomaterials In Vivo

Insufficient vascularization is considered to be one of the main factors limiting the clinical success of tissue-engineered constructs. In order to evaluate new strategies that aim at improving vascularization, reliable methods are required to make the in-growth of new blood vessels into bio-artificial scaffolds visible and quantify the results. Over the past couple of years, our group has introduced a full skin defect model that enables the direct visualization of blood vessels by transillumination and provides the possibility of quantification through digital segmentation. In this model, one surgically creates full skin defects in the back of mice and replaces them with the material tested. Molecules or cells of interest can also be incorporated in such materials to study their potential effect. After an observation time of one&#8217;s own choice, materials are explanted for evaluation. Bilateral wounds provide the possibility of making internal comparisons that minimize artifacts among individuals as well as of decreasing the number of animals needed for the study. In comparison to other approaches, our method offers a simple, reliable and cost effective analysis. We have implemented this model as a routine tool to perform high-resolution screening when testing vascularization of different biomaterials and bio-activation approaches.

A Full Skin Defect Model to Evaluate Vascularization of Biomaterials In Vivo

Vascularization is key to approaches in successful tissue engineering. Therefore, reliable technologies are required to evaluate the development of vascular networks in tissue-constructs. Here we present a simple and cost-effective method to visualize and quantify vascularization in vivo.

Insufficient vascularization is considered to be one of the main factors limiting the clinical success of tissue-engineered constructs. In order to ...

Bioengineering

Isolating and Using Sections of Bovine Mesenteric Artery and Vein as a Bioassay to Test for Vasoactivity in the Small Intestine

Mammalian gastrointestinal systems are constantly exposed to compounds (desirable and undesirable) that can have an effect on blood flow to and from that system. Changes in blood flow to the small intestine can result in effects on the absorptive functions of the organ. Particular interest in toxins liberated from feedstuffs through fermentative and digestive processes has developed in ruminants as an area where productive efficiencies could be improved. The video associated with this article describes an in vitro bioassay developed to screen compounds for vasoactivity in isolated cross-sections of bovine mesenteric artery and vein using a multimyograph. Once the blood vessels are mounted and equilibrated in the myograph, the bioassay itself can be used: as a screening tool to evaluate the contractile response or vasoactivity of compounds of interest; determine the presence of receptor types by pharmacologically targeting receptors with specific agonists; determine the role of a receptor with the presence of one or more antagonists; or determine potential interactions of compounds of interest with antagonists. Through all of this, data are collected real-time, tissue collected from a single animal can be exposed to a large number of different experimental treatments (an in vitro advantage), and represents vasculature on either side of the capillary bed to provide an accurate picture of what could be happening in the afferent and efferent blood supply supporting the small intestine.

The small intestine is frequently exposed to toxins that can influence blood flow and negatively impact nutrient absorption. Using a multimyograph and mesenteric artery and vein isolates, compounds or toxins of interest can be screened for vasoactivity.

Mammalian gastrointestinal systems are constantly exposed to compounds (desirable and undesirable) that can have an effect on blood flow to and from that ...

A Methodological Approach to Non-invasive Assessments of Vascular Function and Morphology

The endothelium is the innermost lining of the vasculature and is involved in the maintenance of vascular homeostasis. Damage to the endothelium may predispose the vessel to atherosclerosis and increase the risk for cardiovascular disease. Assessments of peripheral endothelial function are good indicators of early abnormalities in the vascular wall and correlate well with assessments of coronary endothelial function. The present manuscript details the important methodological steps necessary for the assessment of microvascular endothelial function using laser Doppler imaging with iontophoresis, large vessel endothelial function using flow-mediated dilatation, and carotid atherosclerosis using carotid artery ultrasound. A discussion on the methodological considerations for each of the techniques is also presented, and recommendations are made for future research.

The present article describes the methodological considerations for several non-invasive assessments of vascular function and morphology that are commonly used in medical research to assess different stages of atherosclerosis.

The endothelium is the innermost lining of the vasculature and is involved in the maintenance of vascular homeostasis.  Damage to the endothelium may ...

An Optimized Evans Blue Protocol to Assess Vascular Leak in the Mouse

Vascular leak, or plasma extravasation, has a number of causes, and may be a serious consequence or symptom of an inflammatory response. This study may ultimately lead to new knowledge concerning the causes of or new ways to inhibit or treat plasma extravasation. It is important that researchers have the proper tools, including the best methods available, for studying plasma extravasation. In this article, we describe a protocol, using the Evans blue dye method, for assessing plasma extravasation in the organs of FVBN mice. This protocol is intentionally simple, to as great a degree as possible, but provides high quality data. Evans blue dye has been chosen primarily because it is easy for the average laboratory to use. We have used this protocol to provide evidence and support for the hypothesis that the enzyme neprilysin may protect the vasculature against plasma extravasation. However, this protocol may be experimentally used and easily adapted for use in other strains of mice or in other species, in many different organs or tissues, for studies which may involve other factors that are important in understanding, preventing, or treating plasma extravasation. This protocol has been extensively optimized and modified from existing protocols, and combines reliability, ease of use, economy, and general availability of materials and equipment, making this protocol superior for the average laboratory to use in quantifying plasma extravasation from organs.

In this article, an economical, optimized, and simple protocol is described which uses the Evans blue dye method for assessing plasma extravasation in the organs of FVBN mice that can be adapted for use in other strains, species, and other organs or tissues.

Vascular leak, or plasma extravasation, has a number of causes, and may be a serious consequence or symptom of an inflammatory response. This study may ...

Microperfusion Technique to Investigate Regulation of Microvessel Permeability in Rat Mesentery

Experiments to measure the permeability properties of individually perfused microvessels provide a bridge between investigation of molecular and cellular mechanisms regulating vascular permeability in cultured endothelial cell monolayers and the functional exchange properties of whole microvascular beds. A method to cannulate and perfuse venular microvessels of rat mesentery and measure the hydraulic conductivity of the microvessel wall is described. The main equipment needed includes an intravital microscope with a large modified stage that supports micromanipulators to position three different microtools: (1) a beveled glass micropipette to cannulate and perfuse the microvessel; (2) a glass micro-occluder to transiently block perfusion and enable measurement of transvascular water flow movement at a measured hydrostatic pressure, and (3) a blunt glass rod to stabilize the mesenteric tissue at the site of cannulation. The modified Landis micro-occlusion technique uses red cells suspended in the artificial perfusate as markers of transvascular fluid movement, and also enables repeated measurements of these flows as experimental conditions are changed and hydrostatic and colloid osmotic pressure difference across the microvessels are carefully controlled. Measurements of hydraulic conductivity first using a control perfusate, then after re-cannulation of the same microvessel with the test perfusates enable paired comparisons of the microvessel response under these well-controlled conditions. Attempts to extend the method to microvessels in the mesentery of mice with genetic modifications expected to modify vascular permeability were severely limited because of the absence of long straight and unbranched microvessels in the mouse mesentery, but the recent availability of the rats with similar genetic modifications using the CRISPR/Cas9 technology is expected to open new areas of investigation where the methods described herein can be applied.

The modified Landis technique enables paired measurement of the hydraulic conductivity of individual microvessels in the mesentery of normal and genetically modified rats under control and test conditions using microperfusion techniques. It provides a convenient method to evaluate mechanisms that regulate microvessel permeability and transvascular exchange under physiological conditions.

Experiments to measure the permeability properties of individually perfused microvessels provide a bridge between investigation of molecular and cellular ...

Investigating Novel Mechanisms of Microvascular Dysfunction in Humans

Intradermal Microdialysis: An Approach to Investigating Novel Mechanisms of Microvascular Dysfunction in Humans

The cutaneous vasculature is an accessible tissue that can be used to assess microvascular function in humans. Intradermal microdialysis is a minimally invasive technique used to investigate mechanisms of vascular smooth muscle and endothelial function in the cutaneous circulation. This technique allows for the pharmacological dissection of the pathophysiology of microvascular endothelial dysfunction as indexed by decreased nitric oxide-mediated vasodilation, an indicator of cardiovascular disease development risk. In this technique, a microdialysis probe is placed in the dermal layer of the skin, and a local heating unit with a laser Doppler flowmetry probe is placed over the probe to measure the red blood cell flux. The local skin temperature is clamped or stimulated with direct heat application, and pharmacological agents are perfused through the probe to stimulate or inhibit intracellular signaling pathways in order to induce vasodilation or vasoconstriction or to interrogate mechanisms of interest (co-factors, antioxidants, etc.). The cutaneous vascular conductance is quantified, and mechanisms of endothelial dysfunction in disease states can be delineated.

Author Spotlight: A Pharmacodissection Approach to Uncover Mechanisms in Cardiovascular Disease Risk Populations 

Intradermal microdialysis is a minimally invasive technique used to investigate microvascular function in health and disease. Both dose-response and local heating protocols can be utilized for this technique to explore mechanisms of vasodilation and vasoconstriction in the cutaneous circulation.

The cutaneous vasculature is an accessible tissue that can be used to assess microvascular function in humans. Intradermal microdialysis is a minimally ...

In Vivo Vascular Permeability Detection in Mouse Submandibular Gland

Saliva plays an important role in oral and overall health. The intact endothelial barrier function of blood vessels enables saliva secretion, whereas the endothelial barrier dysfunction is related to many salivary gland secretory disorders. The present protocol describes an in vivo paracellular permeability detection method to evaluate the function of endothelial tight junctions (TJs) in mouse submandibular glands (SMG). First, fluorescence-labeled dextrans with different molecular weights (4 kDa, 40 kDa, or 70 kDa) were injected into the angular veins of mice. Afterward, the unilateral SMG was dissected and fixed in the customized holder under a two-photon laser-scanning microscope, and then images were captured for blood vessels, acini, and ducts. Utilizing this method, the real-time dynamic leakage of the different-sized tracers from blood vessels into the basal sides of the acini and even across the acinar epithelia into the ducts was monitored to evaluate the alteration of the endothelial barrier function under physiological or pathophysiological conditions.

In Vivo Vascular Permeability Detection in Mouse Submandibular Gland

In the present protocol, the endothelial barrier function of the submandibular gland (SMG) was evaluated by injecting different molecular weighted fluorescent tracers into the angular veins of test animal models in vivo under a two-photon laser-scanning microscope.

Saliva plays an important role in oral and overall health. The intact endothelial barrier function of blood vessels enables saliva secretion, whereas the ...

Evaluating Vascular Hyperpermeability-inducing Agents in the Skin with the Miles Assay

Summary

Explore More Videos

Chapters in this video

Assessment of Endothelial Cell Migration After Exposure to Toxic Chemicals

Assessing Tumor Microenvironment of Metastasis Doorway-Mediated Vascular Permeability Associated with Cancer Cell Dissemination using Intravital Imaging and Fixed Tissue Analysis

An in vivo Assay to Test Blood Vessel Permeability

A Full Skin Defect Model to Evaluate Vascularization of Biomaterials In Vivo

Isolating and Using Sections of Bovine Mesenteric Artery and Vein as a Bioassay to Test for Vasoactivity in the Small Intestine

A Methodological Approach to Non-invasive Assessments of Vascular Function and Morphology

An Optimized Evans Blue Protocol to Assess Vascular Leak in the Mouse

Microperfusion Technique to Investigate Regulation of Microvessel Permeability in Rat Mesentery

Intradermal Microdialysis: An Approach to Investigating Novel Mechanisms of Microvascular Dysfunction in Humans

In Vivo Vascular Permeability Detection in Mouse Submandibular Gland