Assessment of Vascular Tone Responsiveness using Isolated Mesenteric Arteries with a Focus on Modulation by Perivascular Adipose Tissues


Your institution must subscribe to JoVE's Biology section to access this content.

Fill out the form below to receive a free trial or learn more about access:



The protocol describes the use of wire myography to evaluate the transmural isometric tension of mesenteric arteries isolated from mice, with special consideration of the modulation by factors released from endothelial cells and perivascular adipose tissues.

Cite this Article

Copy Citation | Download Citations | Reprints and Permissions

Konja, D., Luo, C., Sun, W. Y., Yang, K., Man, A. W., Xu, A., Vanhoutte, P. M., Wang, Y. Assessment of Vascular Tone Responsiveness using Isolated Mesenteric Arteries with a Focus on Modulation by Perivascular Adipose Tissues. J. Vis. Exp. (148), e59688, doi:10.3791/59688 (2019).


Altered vascular tone responsiveness to pathophysiological stimuli contributes to the development of a wide range of cardiovascular and metabolic diseases. Endothelial dysfunction represents a major culprit for the reduced vasodilatation and enhanced vasoconstriction of arteries. Adipose (fat) tissues surrounding the arteries play important roles in the regulation of endothelium-dependent relaxation and/or contraction of the vascular smooth muscle cells. The cross-talks between the endothelium and perivascular adipose tissues can be assessed ex vivo using mounted blood vessels by a wire myography system. However, optimal settings should be established for arteries derived from animals of different species, ages, genetic backgrounds and/or pathophysiological conditions.


Dilatations and constrictions of arteries are achieved by relaxations and contractions, respectively, of their vascular smooth muscle cells. Changes in vascular responsiveness of small arteries contribute to the homeostatic regulation of arterial blood pressure by autonomic nerves and hormones present in the blood (e.g., catecholamines, angiotensin II, serotonin, vasopressin). At the local level, the vascular responses of smooth muscle cells are modulated by signals from both the endothelial cells of the intima and the adipose tissue surrounding the arteries (Figure 1).

The endothelium is not only a passive barrier, but also serves as a surface to exchange signals between the blood and the underlying vascular smooth muscle cells. By releasing various vasoactive substances, the endothelium plays a critical role in the local control of vascular tone responses1. For example, in response to acetylcholine, endothelial nitric oxide synthase (eNOS) is activated in the endothelium to produce nitric oxide (NO), which induces relaxation of the underlying vascular smooth muscle by activating soluble guanylyl cyclase (sGC)2. Other vasoactive substances include the products of cyclooxygenases (e.g., prostacyclin and thromboxane A2), lipoxygenase (e.g., 12-hydroxyeicosatetraenoic acids, 12-HETE), and cytochrome P450 monooxygenases (HETEs and epoxyeicosatrienoic acids, EETs), reactive oxygen species (ROS), and vasoactive peptides (e.g., endothelin-1 and angiotensin II), and endothelium-derived hyperpolarizing factors (EDHF)3. A delicate balance between endothelium-derived vasodilators and vasoconstrictors maintain the local vasomotor tone4,5.

Endothelial dysfunction is characterized by the impairment in endothelium-dependent vasodilatation6, a hallmark of vascular aging7. With age, the ability of endothelium to promote vasodilatation is progressively reduced, due largely to a decreased NO bioavailability, as well as the abnormal expression and function of eNOS in the endothelium and sGC in the vascular smooth muscle cells8,9,10. Reduced NO bioavailability potentiates the production of endothelium-dependent vasoconstrictors11,12. In aged arteries, endothelial dysfunction causes hyperplasia in the media, as reflected by the marked increases in wall thickness, number of medial nuclei, which are reminiscent of the arterial thickening in hypertension and atherosclerosis observed in human patients13,14. In addition, pathophysiological conditions such as obesity, diabetes or hypertension accelerate the development of endothelial dysfunction15,16.

Perivascular adipose tissue (PVAT) releases numerous adipokines to regulate vascular structure and function17. The anti-contractile effect of PVAT is mediated by relaxing factors, such as adiponectin, NO, hydrogen peroxide and hydrogen sulphide18,19,20. However, depending on the location and pathophysiological condition, PVAT also can enhance contractile responses in various arteries21. The pro-contractile substances produced by PVAT include angiotensin-II, leptin, resistin, and ROS22,23.  In most of the studies on isolated blood vessels, PVAT has been considered as a simple structural support for the vasculature and thus removed during the preparation of blood vessel ring segments. Since adipose dysfunction represents an independent risk factor for hypertension and associated cardiovascular complications24, the PVAT surrounding the blood vessels should be considered when investigating the vascular responsiveness of different arteries.

The multi wire myograph systems have been widely used to investigate the vasomotor functions of a variety of blood vessels, including the aorta, mesenteric, renal, femoral, cerebral and coronary arteries25,26. The protocols described herein will use wire myography to evaluate vascular responsiveness in mesenteric arteries isolated from genetically modified mouse models, with a special focus on the modulation by PVAT.

Subscription Required. Please recommend JoVE to your librarian.


All animals used for the following study were provided by the Laboratory Animal Unit of the Faculty of Medicine, The University of Hong Kong. Ethical approval was obtained from the departmental Committee on Use of Laboratory Animals for Teaching and Research (CULATR, no.: 4085-16).

1. Preparations

  1. Preparation of drugs
    1. Store drugs appropriately as stated in the Material Safety Data Sheet (MSDS) immediately after receiving them. Dissolve the drugs in powder form in solvents as high-concentration stock solutions and then aliquot for storage at -20 °C.
      NOTE: Most drugs are dissolved in distilled water to prepare the stock solutions; heating or sonication may be required for some drugs. If drugs do not completely dissolve in water, a drop of 1 M NaOH can be added, while for basic drugs a drop of 1 M HCl can be used. Hydrophobic drugs can be dissolved in dimethylsulfoxide (DMSO) or absolute ethanol. In the latter cases, the final bath concentration (in M) should be known and appropriate controls should be performed to rule out the effects of the solvents.
    2. Prior to experiment, dissolve the drug aliquots (Table of Materials) in Krebs-Ringer Bicarbonate solution (Krebs) containing 115 mM NaCl, 4.6 mM KCl, 2.5 mM CaCl2, 1.17 mM MgSO4, 1.17 mM KH2PO4, 25 mM NaHCO3, 11.1 mM D-glucose and 0.01 mM EDTA, pH 7.4.
    3. For cumulative concentration-response curves, prepare the stocks and working solutions of different drugs by serial dilutions (Table 1).
  2. Setting up the instrument
    1. Calibrate the force transducer for all channels before using the myograph system on each day, or every time the system has been moved.
      NOTE: The detailed calibration procedure varies depending on the model. In general, a two-gram weight is applied to the jaws and the corresponding force should 9.81 ± 0.1 mN. If the reading is off by more than 0.1 mN, the transducer should be re-calibrated. For the system used in the present protocol (see the Table of Materials) the operating values for the force transducer during calibration should be between 3000 and 3500. If the value of the transducer is higher or lower, the force transducer must be replaced.
    2. Adjust and align the mounting supports in each chamber. Continuous and repeated usage of the myograph chamber may cause some misalignment of the mounting support, which needs occasional adjustment before experiments to ensure that the jaws are properly aligned.
      NOTE: Special attention is needed when adjusting the mounting supports as the force transducers are very sensitive and fragile.
    3. Switch on heaters and gas (95% O2 and 5% CO2) at least 30 min before the experiment to allow the chambers and buffers to be warmed up to 37 ± 0.1 °C and equilibrated with the gas mixture.
      1. Check the temperature on the thermometer to ensure the accuracy of the heater. Temperature can be modified to run cooling or warming experiments. If the temperature is not correct as set, apply the offset function of the machine to increase or decrease the settings to reach the required temperature.
    4. At the end of the experiment, clean all chambers and turn off the heater as well as the gas running to the setup.
      1. Do not turn the gas off before all the liquid in the chamber has been sucked out of the system, otherwise the acid/distilled water may regurgitate and reach the organ-chamber during the next use.
      2. To clean the chambers of the wire myograph, the most effective way is to perform acid-wash using a diluted acetic acid solution. Clean the edge and the inside of the chambers with a cotton swab.
      3. After washing, rinse the chambers thoroughly with distilled water. Wipe the outside of the chambers with a wet cloth to remove dried salt. Ethanol can also be used if hydrophobic drugs have been used during the experiment.
      4. An example of the washing procedure is as follows. Fill the chambers with 8% acetic acid solution and incubate for 2 min. Use a cotton-tipped applicator to mechanically clean the steel chamber surface. Avoid any contact with the aluminum part of the myograph.
      5. Aspirate the acetic acid and wash the myograph chamber and supports several times with distilled water and dry the surfaces using absorbent paper or cotton-tip applicators.
  3. Dissection of the mesenteric arterial rings
    NOTE: Animals used for the current study were high-fat diet fed male Adipo-SIRT1 mice and wild type littermates as controls. Each animal weighed approximately 45 g at the time of the experiments.
    1. Euthanize the mouse by intraperitoneal injection of pentobarbital sodium (50 mg/kg).
    2. With surgical scissors and forceps, perform a mid-line laparotomy to reveal the abdominal contents.
    3. Collect the mesenteric arcade into a silicon-coated Petri dish.
    4. Spread and pin down the mesenteric network in the Petri dish to reveal the branching of mesentery and connective tissue meshwork.
    5. Under a microscope (10x), and with fine-scissors and forceps, carefully dissect out surrounding connective tissues. Avoid damaging the adventitial layer. Alternatively, surrounding adipose tissue can be retained around the blood vessel for experiment (if needed).
    6. Using the fine scissors and forceps, excise the secondary branches of mesenteric arteries in ice-cold Krebs buffer.
      NOTE: Each researcher should have his/her own set of dissection kit, strings and stirrups. These tools should be kept properly and cleaned-up every time after the experiment as some drugs are hard to wash away and residue can stick to them.
      1. Keep the blood vessels in cold Krebs buffer while separating the surrounding connective tissues, including PVAT. During handling of the blood vessel, be gentle to prevent unnecessary damage to the endothelium.
      2. If the experiment involves the study of PVAT, retain a 1.5 to 2 mm-diameter sphere of PVAT around the blood vessel. Alternatively, same quantities of adipose tissues can be added in each chamber for experiment.
    7. (Optional) Remove the endothelium from the dissected blood vessel as a control to evaluate the endothelium-dependency of the responses. For mesenteric arteries, remove the endothelium by gently rolling it over a wire stirrup or a hair.
    8. Cut the blood vessel prepared as above into small rings (~2 mm length) and put them in a plastic dish full of aerated (95% O2 and 5% CO2) Krebs buffer for subsequent mounting into the chambers of a wire myograph27.
    9. Transfer the vessel rings into a myograph chamber placed under the microscope. Rings should be placed evenly, with the upper and lower stirrups parallel. The attaching wire (40 µm) should be newly prepared as drugs may bind to the strings.
    10. Thread the blood vessel ring onto a suitable length (2 cm) of the wire and secure to one jaw of the mounting chamber by screwing to fix the position.
    11. Pass a second wire through the ring and anchor to the opposite jaw.
    12. With rings threaded and secured to chamber jaws, mount the chamber onto the myograph setup and turn the micrometer screw clockwise to move the wires close to each other until the force reading on the user interface corresponding to the chamber mounted is zero or just below.
      NOTE: The wire attached to the upper jaw should be of minimal length to ensure that tension can be fully transduced to the detector.
    13. Equilibrate the preparations at 37 °C for at least 30 min prior to the first application of force using the adjustable micrometer.
    14. Assess the tissue viability in 115 mM high potassium (NaCl replaced by KCl on a molar basis) Krebs containing 4.6 mM NaCl, 115 mM KCl, 2.5 mM CaCl2, 1.17 mM MgSO4, 1.17 mM KH2PO4, 25 mM NaHCO3 and 11.1 mM D-glucose at pH 7.4.
      NOTE: Isolated vessels are considered viable if the contractile force transduced and recorded as deflection above the baseline in the data recording software of the myograph system is more than 40% of their resting tone, in response to a contractile agent. If the artery does not contract appropriately, then either the optimal basal tension/wall pressure has not been properly adjusted or the artery may have been damaged during isolation or mounting of the vessel.
    15. (Optional) Assess the integrity of endothelial cells by applying phenylephrine to induce contraction of the vessel to 50% of the initial response to KCl (as recorded by the force transducer in the data recording software), followed by adding 1 µM acetylcholine.
      NOTE: A good blood vessel preparation is crucial for obtaining consistent and accurate results. A preparation should not be used for the experiment either if the endothelial integrity test is unsatisfactory or it does not respond to KCl, indicating that endothelial function or vascular smooth muscle contractility, respectively, are not satisfactory. In this case, the preparation should be replaced with a new ring from the same blood vessel or a new blood vessel.

2. Normalization to determine the optimal initial tension

NOTE: The normalization procedure allows the determination of the optimal internal diameter (IC) of arteries at which the blood vessel experiences a suitable resting transmural pressure (100 mmHg or 13.3 kPa for mesenteric arteries) and produces maximal active forces in response to vasoactive agents.

  1. Switch on the computer and open the data recording software (see the Table of Materials).
  2. Save the experiment as a “LabChart data file” with a new name to avoid overwriting the original setting file.
  3. Open the normalization settings window and set the k factor as 1. Accept the default values for eyepiece calibration (0.3, if vessel length is unknown, or 1 if vessel length is known), target pressure (13.3), online averaging time (2) and delay time (60). Click OK to save the settings.
  4. Select channels of interest and input the wire diameter (40 µm), tissue endpoints (a1: 0; a2: tissue length as measured), initial micrometer reading in the normalization window.
  5. Start the normalization procedure by applying the first passive stretch to the blood vessel (turn the micrometer screw counter-clockwise).
  6. Wait for the vessel to stabilize (3 min) and input the new micrometer reading in the normalization window. The wall tension is automatically calculated and shown as a point on the graph.
    NOTE: The micrometer "steps" used during the passive stretch do not need to be the same. The first few stretches could be 20 µm each. As the stretches get closer to the isobar line, the steps can be reduced to 10 µm, 5 µm, 2 µm or even smaller. Have the main chart window open while adjusting the micrometer settings—if a large spike exceeding the isobar line on a length/tension graph (which indicates points of pressure corresponding to a pre-determined value) appears, reduce the tension.
  7. After each passive stretch, replace the control Krebs with an iso-osmotic high potassium Krebs containing 115 mM KCl. When the contraction reaches a plateau (about 3 min), record the active force (F) by subtracting the passive force at each stretch from the potassium-activated force. Calculate the wall tension as well as the internal circumference (IC) values.
    1. Measure active tension as the deflection above the baseline. The active tension (T) is calculated based on the equation F (mN) = T (mN/mm) x 2 x vessel length (mm). Internal circumference (IC) values are calculated from the micrometer data (IC = 205.6 µm + 2 x “gap”).
  8. Remove the high potassium condition by replacing with fresh Krebs. Repeat washing for three times over 5 min.
  9. Repeat steps 2.5 to 2.8 (by inducing passive stretches followed by active contraction in alternate turns) until the active tension starts to decrease (Figure 2).
  10. After multiple rounds of alternate stretches, the passive length/tension curves give the value of IC100, the internal circumference of the vessel at a transmural pressure of 100 mmHg, as the crossing point with the isobar line.
    NOTE: Each micrometer value during the passive stretches is manually introduced in the software Normalization Module. The program automatically records the corresponding force measurement to generate the passive length/tension curve, which gives the value of IC100 as the crossing point with the isobar line (Figure 2, right panels). The closer the last point is to the isobar line but just above the better normalization is without damaging the vessels. A point too far above the isobar line may physically damage the mounted vessel, causing unreliable results during the experiment.
  11. Create the active length/tension curves to determine IC1 values and calculate the normalization k factor as the ratio of IC1/IC100, which will be used for this type of blood vessel in subsequent myography experiments.
    NOTE: The active length/tension curves are created by plotting the IC values calculated from the micrometer data on the x-axis and active tensions on the y-axis. The IC1 is the value lying within the peak plateau region (red traces in Figure 2, right panels). After plotting the active length/tension curves and determining IC1, the normalization k factor is calculated as the ratio of IC1/IC100. Based on the normalization k factor, the optimal IC for baseline, denoted as IC1, will show on the passive length/tension curve. The micrometer setting for this IC appears under the curve and should be used to set the micropositioner for subsequent myography experiments. The initial tension (T) equals to target pressure (Pi) x IC/2π and the optimal force (F) applied to the vessel equals to T x 2 x vessel length.
  12. Thoroughly wash out the high potassium Krebs and equilibrate the preparations for another 30 to 45 min. Reset the basal tensions to "zero" so that only active contractile responses will be recorded during the subsequent experiment.

3. Phenylephrine-induced contractions

NOTE: Drugs that can be selected for inducing the vasoconstrictive responses include the unspecific adrenoceptor agonist norepinephrine, the selective α-1 adrenoceptor agonist phenylephrine, the peptide hormone angiotensin II, and the monoamine neurotransmitter 5-hydroxytryptamine. Phenylephrine is used in the present protocol for examination (Table of Materials).

  1. Prepare and mount paired arterial rings as described in section 1.3, one with PVAT intact and the other with PVAT removed, from the adjacent sections of each artery for the experiment.
  2. After normalization (described in section 2), pre-contract the arterial segments with high potassium Krebs buffer by adding 115 mM KCl solution to the chamber containing Krebs.
  3. Wait for contraction to plateau (3 min), wash out the high potassium and replace with fresh aerated Krebs buffer. Repeat washing three times over 5 min.
  4. Repeat the KCl stimulation and washing three times and record the maximal contractile response/tension to KCl by subtracting the baseline tension from the tension due to KCl stimulation.
  5. After the last contraction and washing, refill the chamber with warm, aerated Krebs buffer and allow the artery to recover for about 30 min before performing the next task.
  6. To each chamber, add cumulative amounts of phenylephrine (half-log increments from 10-10 to 10-4 M) to induce the concentration-dependent increases in isometric tension of the quiescent preparations.
  7. Start by adding a low concentration of the agonist to the chamber. After allowing enough time for a stable contraction (3–5 min), add the next concentration. Repeat the steps with increasing concentrations of phenylephrine.
  8. After adding the last dose of agonist (phenylephrine), wash out the drug thoroughly and refill the chamber with fresh Krebs buffer. Plot the concentration-dependent responses as increasing percentages of the KCl-induced maximal contractions (Figure 3).
  9. (Optional) To assess the contribution of NO, incubate the preparations with the NO synthase inhibitor, L-NAME (10-4 M), for 30 min prior to the addition of phenylephrine. L-NAME enhances phenylephrine-induced contractions in the quiescent preparations of mesenteric arteries (Figure 4).
    NOTE: The inhibitors or antagonists must have sufficient time to achieve equilibration, usually 30–45 min (be consistent for any set of experiments).
  10. For performing a second concentration-response curve sequentially, wash the chamber completely and repeatedly to remove all of the previous agonists, until no further changes in tone are observed.
    NOTE: Parallel experimentation exposes at least two rings obtained from the same blood vessel to the agonist, one under control conditions and one in the presence of the inhibitor(s); in each ring the concentration-response curve will be performed only once. It is preferred to perform parallel experiments, since this provides a better control for the drug’s action and blood vessel sensitivity. Serial experiments obtain a concentration-response curve to an agonist in a single ring; washing it out, changing the experimental conditions (e.g., adding an inhibitor), and then repeating the concentration response curve on the same ring. In this case, time controls are needed to show that the drug responses are not due to changes of the tissue over time. One can never be certain that the tissue is in exactly the same state after exposure to a concentration-response experiment. Sufficient time (at least 30–60 min) must be given to allow the vessel segments to return to their resting (basal) tension although in some case, this may not occur instantly after dissociation of the high affinity agonist from the receptors. In addition, high potassium Krebs can be applied between the cumulative concentration-response curves to reduce desensitization28. Remember that most antagonists cannot be washed out completely, thus keep adding it for the rest of the experiment.

4. Endothelium-dependent relaxations/contractions

  1. Pre-contract a freshly mounted arterial segment (as described in steps 3.2 to 3.5). Again, record the maximal contractile response/tension to KCl by subtracting the baseline tension from the tension due to KCl stimulation.
  2. (Optional) Incubate the preparations with the NO synthase inhibitor, L-NAME (10-4 M), for 30 min prior to the addition of U46619.
  3. Add the pre-calculated concentrations of U46619 to the chamber and allow a stable, sustained contraction of the artery segments.
    NOTE: Vasodilatory responses are induced in mesenteric arteries pre-contracted to about 80% of the maximal responses to 115 mM KCl. Different agonists can be used to induce contraction by activation of their specific receptors. Here, the blood vessel segments with or without PVAT are pre-contracted with U46619 (1–3 x 10-8 M; Table of Materials), a thromboxane A2 receptor agonist, to induce stable and sustained smooth muscle contractions.
  4. Add cumulative concentrations of acetylcholine (10-10 to 10-4 M) to the organ chamber. Concentration-dependent vasodilatory responses of artery segments are presented as percentage of U46619-induced contractile responses (Figure 5).
    NOTE: For most of the experiment, the next concentration of the relaxing agonist should be added immediately when a plateau is observed to prevent rebound in tension. Concentration-dependent vasodilatory responses of artery segments are normalized as percentage of U46619-induced contractile responses to adjust for minor differences in innervation and diameter between the artery segments (Figure 5).Small variabilities in responsiveness between individual rings obtained from the same blood vessel become minimal when a group of six or more experiments are analyzed statistically. When expressing responses as a percentage of the individual tissue’s own maximal contractions, it is as appropriate to use a paired analysis (e.g., paired Student’s t-test) to compare responses of the same type of tissues from different animals as to compare responses of a single tissue before and after an intervention. When analyzing the effects of PVAT, two-way ANOVA is used followed by multiple-comparison test.
  5. After adding the final dose of the relaxing agonist, remove the drug from each chamber and refill with fresh Krebs buffer. Wash the chamber thoroughly with Krebs buffer and let the artery stabilize for at least 45 min before performing any additional experiments.

Subscription Required. Please recommend JoVE to your librarian.

Representative Results

Examination of the length/tension relationships to obtain the normalization factor k

The amount of stretch applied to a vessel segment influences the extent of the actin-myosin interaction and hence the maximal active force developed. Thus, for every type of blood vessel, determining the amount of stretch needed for maximal active force is required for proper myography studies. Here, normalization of the length/tension relationship is performed for mesenteric arteries isolated from mouse models (Figure 2). The arterial segments were suspended in a four-chamber wire myograph system (see Table of Materials) on stainless steel pins (40 μm diameter). Isometric tension was recorded using an analog-to-digital converter connected to a computer with a recording program. Chambers contained 5 mL of Krebs buffer, kept at 37 °C and aerated with 95% O2 and 5% CO2 to maintain pH at 7.4 throughout the experiment. A passive length/tension relationship was established by incremental stretching of the artery segments until the internal circumference corresponding to 100 mmHg transmural pressure (IC100) was obtained. After each stretch (blue arrows), 115 mM KCl was applied to stimulate contractions (green arrows). The active length/tension curves (red) were plotted by extracting the active force data (subtracting the passive force at each stretch from the KCl-activated force) on the Y-axis and then a graph was created manually with the IC values calculated from the micrometer data on the X-axis. An IC value lying within the peak plateau is IC1 (dashed red lines). The normalization factor k was calculated as IC1/IC100 ratios, which could then be applied to samples of the same vessel type in the subsequent experiment.

Presentation and calculation of concentration-response curves

Most concentration-response curves are performed in a cumulative manner. A low concentration of the agonist is added to the bath (preferably starting with a concentration below the threshold for response). After allowing enough time for a possible response (3-5 min), the next concentration is added. When a response is observed, it is allowed to reach a plateau before the next maximal response is obtained. The half-log (average 3.16-fold) increments in concentration of phenylephrine are applied here to study agonist-induced contractions (Figure 3 and Figure 4).

In most cases, contraction-response curves are not expressed as the raw values of tension/force, but as a percentage of the reference response to KCl obtained at the optimal point of the length/tension curve of the individual blood vessel segment. This adjusts for variability in the size or smooth muscle content of the blood vessel as well as corrects for remodeling changes due to aging or pathology. Here, the maximal contractions induced by 115 mM KCl are obtained at the beginning of the experiment and used for calculating phenylephrine-stimulated contractions of mesenteric arteries with or without PVAT, in the absence or presence of L-NAME (Figure 3 and Figure 4).

To study agonists producing relaxation, the vessels are usually contracted to a uniform level—around 50-80% of the maximal contractile response of that tissue. Since the responses to phenylephrine-induced contractions are different between the experimental groups, the present protocol uses U46619 to stimulate stable contractions before applying the cumulative concentrations of acetylcholine. The smooth muscle relaxation is expressed as a percentage of the initial contraction induced by U46619 (Figure 5).

The concentration-response curves can be compared as the presence of a leftward or rightward shift (e.g., between a control curve and one obtained in the presence of an antagonist) by determining the concentrations producing equal responses, e.g., 30% or 50% of the maximum. These are termed EC30 and EC50, respectively (Figure 3B). Statistical comparison of the mean EC50 values should be performed on the logarithm of their values. Depression of curves is examined by comparing their respective maximal responses (Emax) (Figure 3B). In the examples shown, the phenylephrine-induced contractions in mesenteric arteries were enhanced by L-NAME and the concentration-response curves showed a leftward shift as well as an elevation in the maximal contractions (Figure 4B). The acetylcholine-induced relaxations in mesenteric arteries were inhibited by L-NAME, and the concentration-response curve showed a rightward shift as well as reduction in the maximal relaxations (Figure 5B).

Vascular responses to various pharmacological agents can be computed as the area-under-the-contraction-curve (AUCC) for contractions and area-above-the-relaxation-curve (AARC) for relaxations, respectively, by using the nonlinear logistic regression analysis for comparison10 (Figure 3C, Figure 4C and Figure 5C). The effect of L-NAME can be compared by the values of the AUCC/AARC to determine the NO bioavailability (Figure 6). The basal and stimulated release of NO in mesenteric arteries with or without PVAT can be expressed as the differences in the concentration-response curves of phenylephrine-stimulated contraction (DAUCC) and acetylcholine-induced relaxation (DAARC), respectively, in the presence or absence of L-NAME (Figure 6A and Figure 6B). In the example shown, the presence of PVAT reduced the NO bioavailability in mesenteric arteries collected from mice fed with high fat diet (Figure 6C).

Figure 1
Figure 1: A schematic diagram of the wall structure of arteries. Endothelial cells in the tunica intima mediate endothelium-dependent relaxation/contraction of the vascular smooth muscle, whereas signals released from the perivascular adipose tissue modulates the cross-talks between different layers of the arterial wall. Please click here to view a larger version of this figure.

Figure 2
Figure 2: Representative traces illustrating an experiment to determine the optimal initial tensions for mouse mesenteric arteries. The blood vessel segments were prepared from mesenteric arteries collected from the 16-week-old mice fed with standard chow (A) or high fat diet (B). After mounting, the passive and active length/tension curves were obtained by step-wise stretching and sequential stimulation with 115 mM KCl (left panels). The active contraction generated with each stimulation should increase as the vessel is progressively stretched, until it reaches a plateau at the optimal length. Further stretch will lead to a decrease in the active contraction. The IC100 and IC1 were determined by plotting the passive and active length/tensions curves, respectively (right panels). Note that the passive length/tension curve was generated by the Normalization Module after manually inputting the micrometer values, whereas the active length/tensions curves plotted manually after calculating the tension and IC values at each step of KCl stimulation. The IC1/IC100 ratios were calculated as normalization k factor (right panels). ). Note also that only the last four points of the active length/tension curve were shown in the figures in panel (B). STC: Standard chow fed mouse artery; HFD: High-fat diet fed mouse artery. Please click here to view a larger version of this figure.

Figure 3
Figure 3: Output recordings of the vasoconstrictor responses to phenylephrine in mesenteric arteries with or without surrounding PVAT. Contractility studies are performed on preparations of mesenteric arteries from 16-week-old Adipo-SIRT1 transgenic mice, in which the human SIRT1 is overexpressed selectively in adipose tissues29. Cumulative concentrations of phenylephrine were applied to stimulate the contractions of mesenteric arteries without (-PVAT) or with (+PVAT), (A). The contractile responses were recorded and calculated as percentage of 115 mM KCl-induced maximal contraction (B). The area-under-the contraction curves (AUCC) were plotted for comparison (C). Note that PVAT from Adipo-SIRT1 mice elicited an anti-contractile effect on the response to phenylephrine. Please click here to view a larger version of this figure.

Figure 4
Figure 4: Output recordings of the vasoconstrictor responses to phenylephrine in mesenteric arteries with or without the surrounding PVAT, and in the absence or presence of L-NAME. Mesenteric arteries were collected from 16-week-old wild type mice fed with high fat diet. Thirty min after adding 10-4 M L-NAME or vehicle control, cumulative concentrations of phenylephrine were applied to stimulate the contractions of mesenteric arteries (A). The contractile responses were recorded and calculated as percentage of 115 mM KCl-induced maximal contraction (B). The area-under-the contraction curves (AUCC) were plotted for comparison (C). Note that PVAT from dietary obese mice did not elicit anti-contractile effects on the response to phenylephrine. –PVAT: arterial rings prepared without PVAT; +PVAT: arterial rings prepared with the surrounding PVAT; -L-NAME: arterial rings not incubated with L-NAME; +L-NAME: arterial rings incubated with L-NAME. Please click here to view a larger version of this figure.

Figure 5
Figure 5: Output recordings of the vasodilator responses to acetylcholine in mesenteric arteries with or without the surrounding PVAT, and in the absence or presence of L-NAME. Mesenteric arteries were collected from 16-week-old mice fed with high fat diet. At 30 min after adding 10-4 M L-NAME or vehicle control, the blood vessel segments with or without PVAT are pre-contracted with U46619 (1­-3 x 10-8 M; Table of Materials), a thromboxane A2 receptor agonist, to induce stable and sustained smooth muscle contractions. Cumulative concentrations of acetylcholine were then applied to stimulate the relaxations of mesenteric arteries with or without the surrounding PVAT (A). The relaxation responses were recorded and calculated as percentage of U46619-induced contraction (B). The area-above-the relaxation curves (AARC) were plotted for comparison (C). Note that only the arterial segment with surrounding PVAT is shown in panel A. –PVAT: arterial rings prepared without PVAT; +PVAT: arterial rings prepared with the surrounding PVAT; -L-NAME: arterial rings not incubated with L-NAME; +L-NAME: arterial rings incubated with L-NAME. Please click here to view a larger version of this figure.

Figure 6
Figure 6: Illustration of the procedure to calculate NO bioavailability. The area-under-the-contraction-curves (AUCC) and the area-above-the-relaxation-curves (AARC) were calculated based on the responses to cumulative concentrations of phenylephrine (A) and acetylcholine (B), respectively. The differences between preparations pre-treated without and with L-NAME were defined as ∆AUCC (A) and ∆ AARC (B) to represent basal NO contribution and stimulated NO release, respectively. Accordingly, the ∆AUCC (calculated from Figure 4C), ∆AARC (calculated from Figure 5C), and the sum of both (total NO bioavailability) were presented for comparing the NO bioavailability in mesenteric arteries without and with the surrounding PVAT (C). –PVAT: arterial rings prepared without PVAT; +PVAT: arterial rings prepared with the surrounding PVAT; -L-NAME: arterial rings not incubated with L-NAME; +L-NAME: arterial rings incubated with L-NAME. Please click here to view a larger version of this figure.

Subscription Required. Please recommend JoVE to your librarian.


Apart from the endothelial cells, signals derived from PVAT play an important role in the regulation of smooth muscle tone reactivity30. Healthy PVAT releases NO and anti-inflammatory adiponectin to exert an anti-contractile effect on arteries, which is lost under pathological conditions such as obesity and metabolic syndrome31,32. In disease states, PVAT contributes to the development of endothelial dysfunction and other cardiovascular abnormalities33,34. Abnormal eNOS expression and function have been reported in PVAT of arteries from obese animals35,36. Since both endothelial and PVAT dysfunctions contribute to the development of cardiovascular and metabolic abnormalities23,37, when performing ex vivo vascular experiment, their role should be considered by including in or removing them from the preparations.

The wire myography system provides a convenient platform to dissect the vasoactive signals released from PVAT using different pharmacological probes10,38. However, the compositions in PVAT of different types of arteries, or the same arteries from animals of different genetic background, are not same39. Therefore, the wire myography results involving PVAT should not be compared across different types of arteries or the same type of arteries from mice of different strains. Age and the underlying disease states also affect the cellular compositions in PVAT. Here, mice from the same genetic background but with different genetic modifications in their adipose tissue were used for comparing the vasomodulating activity of PVAT.

As a main source of resistance to blood flow, mesenteric arteries are chosen for the present study. Resting tension determines the amount of vasomotor responsiveness40. The optimal initial tension of the blood vessel is affected by the type of artery, age, diet, treatment and genetic background of the animals, thus should be determined individually before examining relaxation/contraction-response curves. For the present demonstration, the superior mesenteric arteries were collected from 16-week-old mice fed with standard chow or high fat diet starting from the age of four weeks. The present protocol emphasizes the establishment of optimal settings for maximal active force production of the arterial segments before assessing pharmacological responses. Both passive and active length/tension relationships are studied for mesenteric arteries collected from in-house mouse models. A normalization k factor of 1 has been established for preparations from the 16-week-old animals, which is different from the default value of 0.9 or those used by previous publications41. Caution is needed when comparing the normalization ratios in the literature due to possible differences in the technique, buffer composition and instrument models, etc.  In particular, age, diet and other pathophysiological conditions affect the passive and active tension as well as the pharmacodynamics characteristics of arteries42.

Subscription Required. Please recommend JoVE to your librarian.


Authors have nothing to disclose.


This work was financially support by the grants from Research Grant Council of Hong Kong [17124718 and 17121714], Hong Kong Health and Medical Research Fund [13142651 and 13142641], Collaborative Research Fund of Hong Kong [C7055-14G], and the National Basic Research Program of China [973 Program 2015CB553603].


Name Company Catalog Number Comments
Acetylcholine Sigma-Aldrich A6625 Stock concentration: 10-1 M
Working concentration: 10-10 to 10-5 M
L-NAME (Nω-nitro-L-arginine methyl ester) Sigma-Aldrich N5751 Stock concentration: 3 x 10-2 M
Working concentration: 10-4 M
Phenylephrine Sigma-Aldrich P6126 Stock concentration: 10-2 M
Working concentration: 10-10 to 10-5 M
U46619 (9,11-dideoxy-9α,11αmethanoepoxy prostaglandin F2α) Enzo BML-PG023-0001 Stock concentration: 10-5 M
Working concentration: 1-3 x 10-8 M
Multiwire myograph Danish MyoTechnology (DMT) 620M
PowerLab 4/26 ADInstruments ML848
Labchart7 ADInstruments -
Adipo-SIRT1 wild type mice Laboratory Animal Unit, The University of Hong Kong CULATR NO.: 4085-16
Silicon-coated Petri dishes Danish MyoTechnology (DMT)
Tungsten wires Danish MyoTechnology (DMT) 300331
Surgical tools



  1. Furchgott, R. F., Zawadzki, J. V. The obligatory role of endothelial cells in the relaxation of arterial smooth muscle by acetylcholine. Nature. 288, (5789), 373-376 (1980).
  2. Furchgott, R. F., Vanhoutte, P. M. Endothelium-derived relaxing and contracting factors. The FASEB Journal. 3, (9), 2007-2018 (1989).
  3. Feletou, M., Kohler, R., Vanhoutte, P. M. Endothelium-derived vasoactive factors and hypertension: possible roles in pathogenesis and as treatment targets. Current Hypertension Reports. 12, (4), 267-275 (2010).
  4. Vanhoutte, P. M. Endothelial dysfunction: the first step toward coronary arteriosclerosis. Circulation Journal. 73, (4), 595-601 (2009).
  5. Feletou, M., Huang, Y., Vanhoutte, P. M. Endothelium-mediated control of vascular tone: COX-1 and COX-2 products. British Journal of Pharmacology. 164, (3), 894-912 (2011).
  6. Harrison, D. G. Cellular and molecular mechanisms of endothelial cell dysfunction. Journal of Clinical Investigation. 100, (9), 2153 (1997).
  7. Vanhoutte, P. M., Shimokawa, H., Tang, E. H., Feletou, M. Endothelial dysfunction and vascular disease. Acta physiologica. 196, (2), 193-222 (2009).
  8. Klöß, S., Bouloumié, A., Mülsch, A. Aging and chronic hypertension decrease expression of rat aortic soluble guanylyl cyclase. Hypertension. 35, (1), 43-47 (2000).
  9. Csiszar, A., et al. Aging-induced phenotypic changes and oxidative stress impair coronary arteriolar function. Circulation Research. 90, (11), 1159-1166 (2002).
  10. Guo, Y., et al. Endothelial SIRT1 prevents age-induced impairment of vasodilator responses by enhancing the expression and activity of soluble guanylyl cyclase in smooth muscle cells. Cardiovascular Research. (2018).
  11. Auch-Schwelk, W., Katusic, Z. S., Vanhoutte, P. M. Nitric oxide inactivates endothelium-derived contracting factor in the rat aorta. Hypertension. 19, (5), 442-445 (1992).
  12. Tang, E. H., Feletou, M., Huang, Y., Man, R. Y., Vanhoutte, P. M. Acetylcholine and sodium nitroprusside cause long-term inhibition of EDCF-mediated contractions. American Journal of Physiology - Heart and Circulation Physiology. 289, (6), H2434-H2440 (2005).
  13. Ghiadoni, L., et al. Endothelial function and common carotid artery wall thickening in patients with essential hypertension. Hypertension. 32, (1), 25-32 (1998).
  14. Xu, X., et al. Age-related Impairment of Vascular Structure and Functions. Aging and Disease. 8, (5), 590-610 (2017).
  15. Tabit, C. E., Chung, W. B., Hamburg, N. M., Vita, J. A. Endothelial dysfunction in diabetes mellitus: Molecular mechanisms and clinical implications. Reviews in Endocrine & Metabolic Disorders. 11, (1), 61-74 (2010).
  16. Tanaka, K., Sata, M. Roles of perivascular adipose tissue in the pathogenesis of atherosclerosis. Frontiers in Physiology. 9, 3 (2018).
  17. Brown, N. K., et al. Perivascular adipose tissue in vascular function and disease: a review of current research and animal models. Arteriosclerosis Thrombosis and Vascular Biology. 34, (8), 1621-1630 (2014).
  18. Lohn, M., et al. Periadventitial fat releases a vascular relaxing factor. The FASEB Journal. 16, (9), 1057-1063 (2002).
  19. Gálvez-Prieto, B., et al. A reduction in the amount and anti-contractile effect of periadventitial mesenteric adipose tissue precedes hypertension development in spontaneously hypertensive rats. Hypertension research. 31, (7), 1415 (2008).
  20. Gao, Y. J., Lu, C., Su, L. Y., Sharma, A., Lee, R. Modulation of vascular function by perivascular adipose tissue: the role of endothelium and hydrogen peroxide. British Journal of Pharmacology. 151, (3), 323-331 (2007).
  21. Gao, Y. -J., et al. Perivascular adipose tissue promotes vasoconstriction: the role of superoxide anion. Cardiovascular Research. 71, (2), 363-373 (2006).
  22. Szasz, T., Webb, R. C. Perivascular adipose tissue: more than just structural support. Clinical Science (London). 122, (1), 1-12 (2012).
  23. Ramirez, J. G., O'Malley, E. J., Ho, W. S. V. Pro-contractile effects of perivascular fat in health and disease. Brish Journal of Pharmacology. 174, (20), 3482-3495 (2017).
  24. Hajer, G. R., van Haeften, T. W., Visseren, F. L. Adipose tissue dysfunction in obesity, diabetes, and vascular diseases. European Heart Journal. 29, (24), 2959-2971 (2008).
  25. Mulvany, M. J., Halpern, W. Contractile properties of small arterial resistance vessels in spontaneously hypertensive and normotensive rats. Circulation Research. 41, (1), 19-26 (1977).
  26. Mulvany, M. J., Halpern, W. Mechanical properties of vascular smooth muscle cells in situ. Nature. 260, (5552), 617-619 (1976).
  27. del Campo, L., Ferrer, M. Wire myography to study vascular tone and vascular structure of isolated mouse arteries. Methods in Molecular Biology. 1339, 255-276 (2015).
  28. Dobrin, P. B. Influence of initial length on length-tension relationship of vascular smooth muscle. American Journal of Physiology. 225, (3), 664-670 (1973).
  29. Xu, C., et al. Calorie restriction prevents metabolic aging caused by abnormal SIRT1 function in adipose tissues. Diabetes. 64, (5), 1576-1590 (2015).
  30. Sheykhzade, M., Nyborg, N. C. Caliber dependent calcitonin gene-related peptide-induced relaxation in rat coronary arteries: effect of K+ on the tachyphylaxis. European Journal of Pharmacology. 351, (1), 53-59 (1998).
  31. Soltis, E. E., Cassis, L. A. Influence of perivascular adipose tissue on rat aortic smooth muscle responsiveness. Clinical and Experimental Hypertension A. 13, (2), 277-296 (1991).
  32. Lohn, M., et al. Periadventitial fat releases a vascular relaxing factor. FASEB Journal. 16, (9), 1057-1063 (2002).
  33. Fesus, G., et al. Adiponectin is a novel humoral vasodilator. Cardiovascular Research. 75, (4), 719-727 (2007).
  34. Greenstein, A. S., et al. Local inflammation and hypoxia abolish the protective anticontractile properties of perivascular fat in obese patients. Circulation. 119, (12), 1661-1670 (2009).
  35. Yudkin, J. S., Eringa, E., Stehouwer, C. D. "Vasocrine" signalling from perivascular fat: a mechanism linking insulin resistance to vascular disease. Lancet. 365, (9473), 1817-1820 (2005).
  36. Xia, N., et al. Uncoupling of endothelial nitric oxide synthase in perivascular adipose tissue of diet-induced obese mice. Arteriosclerosis Thrombosis and Vascular Biology. 36, (1), 78-85 (2016).
  37. Xia, N., Forstermann, U., Li, H. Effects of resveratrol on eNOS in the endothelium and the perivascular adipose tissue. Annals of the New York Academy of Sciences. 1403, (1), 132-141 (2017).
  38. Schinzari, F., Tesauro, M., Cardillo, C. Endothelial and perivascular adipose tissue abnormalities in obesity-related vascular dysfunction: novel targets for treatment. Journal of Cardiovascular Pharmacology. 69, (6), 360-368 (2017).
  39. Liu, J. T., et al. Lipocalin-2 deficiency prevents endothelial dysfunction associated with dietary obesity: role of cytochrome P450 2C inhibition. British Journal of Pharmacology. 165, (2), 520-531 (2012).
  40. Martinez-Quinones, P., et al. Hypertension induced morphological and physiological changes in cells of the arterial wall. American Journal of Hypertension. 31, (10), 1067-1078 (2018).
  41. Outzen, E. M., et al. Translational value of mechanical and vasomotor properties of mouse isolated mesenteric resistance-sized arteries. Pharmacology Research and Perspectives. 3, (6), e00200 (2015).
  42. Sheykhzade, M., Simonsen, A. H., Boonen, H. C., Outzen, E. M., Nyborg, N. C. Effect of ageing on the passive and active tension and pharmacodynamic characteristics of rat coronary arteries: age-dependent increase in sensitivity to 5-HT and K+. Pharmacology. 90, (3-4), 160-168 (2012).



    Post a Question / Comment / Request

    You must be signed in to post a comment. Please or create an account.

    Usage Statistics