Skeletal Muscle Neurovascular Coupling, Oxidative Capacity, and Microvascular Function with 'One Stop Shop' Near-infrared Spectroscopy

JoVE Journal

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

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



Here, we describe a simple, non-invasive approach using near-infrared spectroscopy to assess reactive hyperemia, neurovascular coupling and skeletal muscle oxidative capacity in a single clinic or laboratory visit.

Cite this Article

Copy Citation | Download Citations | Reprints and Permissions

Rosenberry, R., Chung, S., Nelson, M. D. Skeletal Muscle Neurovascular Coupling, Oxidative Capacity, and Microvascular Function with 'One Stop Shop' Near-infrared Spectroscopy. J. Vis. Exp. (132), e57317, doi:10.3791/57317 (2018).


Exercise represents a major hemodynamic stress that demands a highly coordinated neurovascular response in order to match oxygen delivery to metabolic demand. Reactive hyperemia (in response to a brief period of tissue ischemia) is an independent predictor of cardiovascular events and provides important insight into vascular health and vasodilatory capacity. Skeletal muscle oxidative capacity is equally important in health and disease, as it determines the energy supply for myocellular processes. Here, we describe a simple, non-invasive approach using near-infrared spectroscopy to assess each of these major clinical endpoints (reactive hyperemia, neurovascular coupling, and muscle oxidative capacity) during a single clinic or laboratory visit. Unlike Doppler ultrasound, magnetic resonance images/spectroscopy, or invasive catheter-based flow measurements or muscle biopsies, our approach is less operator-dependent, low-cost, and completely non-invasive. Representative data from our lab taken together with summary data from previously published literature illustrate the utility of each of these end-points. Once this technique is mastered, application to clinical populations will provide important mechanistic insight into exercise intolerance and cardiovascular dysfunction.


The hyperemic response to a brief period of tissue ischemia has emerged as a key non-invasive measure of (micro)vascular function. During occlusion of a conduit artery, downstream arterioles dilate in an effort to offset the ischemic insult. Upon release of the occlusion, the decreased vascular resistance results in hyperemia, the magnitude of which is dictated by one's ability to dilate the downstream microvasculature. While reactive hyperemia is a strong independent predictor of cardiovascular events1,2 and therefore a clinically significant endpoint, its functional significance to exercise tolerance and quality of life is less clear.

Indeed, dynamic exercise represents a major cardiovascular stress that demands a highly coordinated neurovascular response in order to match oxygen delivery to metabolic demand. For example, skeletal muscle blood flow can increase nearly 100-fold during isolated muscle contractions3, which would overwhelm the pumping capacity of the heart if such a hemodynamic response were extrapolated to whole-body exercise. Accordingly, to avoid severe hypotension, sympathetic (i.e., vasoconstrictor) nervous activity increases to redistribute cardiac output away from inactive and visceral tissues and towards active skeletal muscle4. Sympathetic outflow is also directed to the exercising skeletal muscle5; however, local metabolic signaling attenuates the vasoconstrictor response in order to ensure adequate tissue oxygen delivery6,7,8,9,10,11. Collectively, this process is termed functional sympatholysis12, and is imperative to the normal regulation of skeletal muscle blood flow during exercise. Since skeletal muscle blood flow is a key determinant of aerobic capacity — an independent predictor of quality of life and cardiovascular disease morbidity and mortality13— understanding the control of skeletal muscle blood flow and tissue oxygen delivery during exercise is of great clinical significance.

Oxygen delivery is only half of the Fick equation, however, with oxygen utilization satisfying the other half of the equation. Among the major determinates of oxygen utilization, mitochondrial oxidative phosphorylation plays an essential role in supplying adequate energy for cellular processes both at rest and during exercise. Indeed, impairments in muscle oxidative capacity can limit functional capacity and quality of life14,15,16. Various measures are commonly used to provide an index of muscle oxidative capacity, including invasive muscle biopsies and expensive and time-consuming magnetic resonance spectroscopy (MRS) techniques.

Here, we propose a novel, non-invasive approach, using near-infrared spectroscopy (NIRS), to assess each of these three major clinical endpoints (reactive hyperemia, sympatholysis, and muscle oxidative capacity) in a single clinic or laboratory visit. The major advantages of this approach are three-fold: First, this technique is easily portable, relatively low cost, and easy to perform. Current Doppler ultrasound approaches for measuring reactive hyperemia are highly operator-dependent — requiring extensive skill and training — and require sophisticated, high-cost, data acquisition hardware and post-processing software. Moreover, this could conceivably be introduced into the clinic and/or large clinical trials for bedside monitoring or testing therapeutic efficacy. Second, by virtue of the methodology, this technique focuses specifically on the skeletal muscle microvasculature, increasing the overall specificity of the technique. Alternative approaches using Doppler ultrasound focus entirely on upstream conduit vessels and infer changes downstream, which can dampen the signal. Third, this technique is completely non-invasive. Skeletal muscle oxidative capacity is traditionally assessed with invasive and painful muscle biopsies, and functional sympatholysis may be assessed with intra-arterial injection of sympathomimetics and sympatholytics. This approach avoids these requirements all together.

Subscription Required. Please recommend JoVE to your librarian.


This protocol follows the guidelines of the institutional review board at the University of Texas at Arlington and conforms to the standards set by the latest version of the Declaration of Helsinki. Accordingly, written informed consent was (and should be) obtained prior to commencement of research procedures.

1. Instrumentation

NOTE: The following instrumentation description is based on the near-infrared (NIR) spectrometer and data acquisition system used in our lab (see Table of Materials). Thus, the instructions include steps that are necessary for the optimal function of these devices. These steps include the calibration of the NIR probe using the accompanying software and calibration phantom, and the application of a dark cloth to exclude ambient light. In the event that different data collection hardware and/or software are used, investigators should consult their own specific user manuals for calibration and ambient light considerations. Figure 1 illustrates the experimental set-up and instrumentation described immediately below.

  1. Instruct the subject to lie supine with their legs inside a lower body negative pressure (LBNP) chamber (Figure 1A), so that their belt line is approximately even with the opening to the LBNP box. For instructions on how to build a LBNP chamber, see References17.
  2. Place three electrocardiogram electrodes on the subject: two in an inferior, mid-clavicular location and one on the subject's left side medial to the iliac crest. This configuration provides the best results due to limited access to the lower limbs, instrumentation of the upper limbs, and arm movement during hand grip exercise.
  3. Place a non-invasive blood pressure monitor module on the subject's dominant wrist. Place the finger blood pressure cuffs on each finger and connect them to the module (Figure 1B). Ensure the finger blood pressure cuffs are properly calibrated according to the user's manual accompanying your device.
  4. Instruct the subject to grasp a hand grip dynamometer (HGD) with their non-dominant arm in a slightly abducted position. The arm should be comfortably positioned on a bedside table. The distance and angle of the HGD should be adjusted to allow for optimal grip strength with minimal arm movement (Figure 1C).
  5. Secure the HGD to a bedside table.
  6. Measure the maximum voluntary contraction (MVC) of the participant. Tell the participant that, when prompted, they must squeeze the HGD as hard as possible while only utilizing the muscles in the hand and forearm. Instruct the subject that they must refrain from recruiting their upper arm, chest, shoulder, or abdominal muscles when performing the maximum grip.
  7. Repeat Step 1.6 three times, separated by at least 60 s. Record the maximum force achieved (best of 3). This maximum force will be used to calculate the exercise intensity for skeletal muscle oxidative capacity and neurovascular coupling (below).
  8. Place a rapid-inflation cuff around the upper arm of the exercising hand. Connect the airline from the rapid inflation controller to the cuff.
  9. Identify the flexor digitorum profundus. Use a skin marker to demarcate the borders of the palpable muscle.
  10. Ensure that the NIR spectrometer is properly calibrated according to the user's manual included with your device. Clean the skin over which the NIR probe will be positioned with an alcohol prep wipe.
  11. Place the NIR probe over the center of the belly of the muscle (flexor digitorum profundus) and affix it securely to the forearm.
  12. Wrap the probe and forearm with dark cloth, minimizing interference from ambient light (Figure 1C, Figure 1D).
  13. When ready to perform the functional sympatholysis portion of the study, seal the subject into the LBNP chamber.

2. Skeletal Muscle Oxidative Capacity

NOTE: A representative data tracing illustrating the experimental procedure for measuring skeletal muscle oxidative capacity is depicted in Figure 2. This experimental approach has previously been validated against in vivo phosphorus MRS18 and in situ muscle respirometry19, and is gaining widespread acceptance20.

  1. Instrument the subject as indicated above (Instrumentation).
  2. Instruct the subject to lie still for 2 min while monitoring deoxyhemoglobin (HHb) and oxyhemoglobin (HbO2) via the NIR probe.
    NOTE: This rest period allows the subject to recover from any movement artifact associated with the instrumentation process, and ensures stable baseline measurements. If after 2 min no significant fluctuations have occurred, the subject may be considered at a steady state, or resting baseline.
  3. Prior to cuff occlusion, notify your subject that you will be inflating the cuff. Inflate the upper arm cuff at least 30 mmHg above systolic blood pressure for 5 min (i.e., suprasystolic). Instruct the subject to keep their arm as still and relaxed as possible both during cuff inflation and following cuff deflation.
    NOTE: This 5 min brachial artery cuff occlusion protocol closely reflects the currently accepted clinical standard for vascular occlusion tests21,22,23,24,25.
  4. Record the initial/baseline value (prior to cuff occlusion) and the nadir value of tissue saturation (StO2) during the cuff occlusion and determine the midpoint between these two values.
    Equation 1
  5. Allow the subject to recover from the cuff occlusion and return to the resting baseline values. Once the subject has maintained a resting baseline for at least 1 full min, continue to the next step.
  6. Instruct subject to squeeze and maintain an isometric hand grip at 50% of their MVC. Encourage the subject to maintain their isometric contraction until the tissue desaturates by 50%. Upon achieving this value, tell the subject to relax their hand and inform them that no more exercise or movement is needed.
  7. Within 3 - 5 s following exercise cessation, administer the following rapid cuff occlusion series (one series = 1 inflation + 1 deflation), as previously established18:
    Series #1 - 6: 5 s on/5 s off
    Series #7 - 10: 7 s on/10 s off
    Series #11 - 14: 10 s on/15 s off
    Series #15 - 18: 10 s on/20 s off
  8. After completing the 18th inflation/deflation series, instruct the subject to rest, allowing tissue saturation to return to initial baseline values. After these values have remained consistent for at least 2 min, repeat steps 2.4 and 2.5.
  9. Calculating Skeletal Muscle Oxidative Capacity
    1. Calculate the slope of change in the StO2for each of the individual 18 cuff occlusions, forming the monoexponential recovery points illustrated in Figure 2C.
    2. Fit the calculated data from 2.7 to the following monoexponential curve18,19,26
      y = End - Δ x e-kt
      NOTE: 'y' is the relative muscle oxygen consumption rate (mV̇O2) during cuff inflation, 'End' represents the mV̇O2 immediately following the cessation of exercise; delta ('Δ') signifies the change in mV̇O2 from rest to the end of exercise; 'k' is the fitting rate constant; 't' is time. Tau is calculated as 1/k.

3. Reactive Hyperemia

NOTE: A representative data tracing illustrating the experimental procedure for measuring reactive hyperemia is depicted in Figure 3.

  1. With the subject lying supine and instrumented as described above (Instrumentation), instruct the subject to lie as still as possible.
  2. Once the subject has achieved a consistent resting state, continue to record at least 1 min of baseline data and then rapidly inflate a blood pressure cuff on the upper arm to a suprasystolic pressure (30 mmHg above systolic blood pressure).
  3. At the 5 min mark, rapidly deflate the cuff while recording the hyperemic response.
  4. Continue recording for at least 3 min to capture the subject's recovery.
  5. Calculating Reactive Hyperemia
    NOTE: The NIRS parameters calculated are depicted in Figure 3.
    1. Calculate baseline StOas the average StOover 1 full min prior to the onset of arterial cuff occlusion.
    2. Determine the resting skeletal muscle metabolic rate as the desaturation rate (i.e., average slope) during cuff occlusion (defined as Slope 1)27,28.
    3. Calculate reactive hyperemia as follows:
      a) the average upslope following cuff release (i.e., reperfusion rate, defined as slope 2), calculated from the moment of cuff release through the linearly increasing phase of the rebound trace;
      b) the highest StOvalue reached after cuff release (denoted as StO2max);
      c) the reactive hyperemia area under the curve (AUC); calculated from the time of cuff release to 1-, 2- and 3-min post cuff-occlusion (AUC 1-min, AUC 2-min, and AUC 3-min, respectively); and
      d) the hyperemic reserve, calculated as the change in StOabove baseline and reported as a percent (%) change. This value is calculated as the highest saturation achieved during the post-occlusive rebound minus the average saturation calculated in step 3.5.1 (see above).
      NOTE: Large differences in baseline data will greatly affect the interpretation of the hyperemic reserve.

4. Functional Sympatholysis

NOTE: A representative data tracing illustrating the experimental procedure for measuring functional sympatholysis is depicted in Figure 4.

  1. Instrument the subject as indicated above (Instrumentation).
  2. Ensure an airtight seal in the LBNP chamber.
  3. With the subject lying still and at rest, collect 3 min of baseline data.
  4. At the 3 min mark, turn on the vacuum. Adjust the vacuum so that the pressure inside the LBNP chamber is between -20 and -30 mmHg. Allow the vacuum to run for 2 min while monitoring the subject's response.
  5. At the 5 min mark, turn off the vacuum and allow the subject to rest for 3 min.
  6. At the 8 min mark, initiate the voice prompt guiding the subject through the rhythmic hand grip exercise (20% MVC).
  7. Confirm that the subject is maintaining their squeeze throughout the entirety of each gripping phase and relaxing completely during between each repetition. Monitor their force output and confirm that they are achieving 20% MVC with each grip. Continue exercise until the 11 min mark.
  8. At the 11 min mark, turn on the vacuum encouraging the subject to continue their rhythmic exercise. Allow the vacuum to run from 11 - 13 min, then turn it off.
  9. Have the subject continue performing rhythmic hand grip exercise at 20% of their MVC for an additional 2 min. Upon exercise cessation, have the subject rest quietly and lie still.
  10. Calculating Functional Sympatholysis
    1. Normalize the change in oxyhemoglobin with LBNP to the total labile signal (TLS), determined during 5 min cuff occlusion:
      Equation 2
      Equation 3
    2. Calculate each event as the final 20 min average of each event.
    3. Calculate the exercise-induced attenuation of the oxyhemoglobin reduction:
      Equation 4

Subscription Required. Please recommend JoVE to your librarian.

Representative Results

Skeletal muscle oxidative capacity

Figure 2 illustrates a representative participant response during a NIRS-derived skeletal muscle oxidative capacity assessment. Panel A shows the tissue saturation profile during a 5 min arterial cuff occlusion protocol, handgrip exercise, and intermittent arterial occlusion during recovery from exercise. Panel B illustrates the expected tissue desaturation/re-saturation profile during the intermittent arterial occlusions during the recovery period. The rate of desaturation is directly proportional to the rate of muscle oxygen consumption, and is plotted in Panel C for each of the intermittent cuff occlusion periods. The calculated muscle oxygen consumption recovery data is then fit to a monoexponential curve and the recovery time constant derived. Using the same approach, a growing number of studies have evaluated skeletal muscle oxidative capacity for both health and disease, across a variety of muscle groups (Table 1).

Reactive Hyperemia

Figure 3 illustrates the NIRS-derived reactive hyperemia profile during a representative vascular occlusion test. This same approach has been used across a wide range of study populations and muscle groups with good success (Table 2). The data indicate that NIRS-derived reactive hyperemia not only provides valuable insight into vascular reactivity, but that the test is easily adaptable and clinically meaningful.

Functional Sympatholysis

Table 3 summarizes the existing literature using the exact same neurovascular coupling approach described herein to measure functional sympatholysis, showing both mechanistic and clinically relevant outcomes. In healthy control subjects, when LBNP is superimposed on mild handgrip, the reflex decrease in muscle oxygenation is attenuated by ~50% (Figure 4). Failure to attenuate sympathetic (vasoconstrictor) nerve activity during exercise, as with cardiovascular or neurological disease (Table 3), disrupts the balance between oxygen delivery and utilization, and causes functional muscle ischemia.

Figure 1
Figure 1. Experimental set-up and instrumentation. (A) Representative experimental set-up, with a typical subject lying supine on a bed with their legs inside the LBNP chamber and fully instrumented. (B) Dominant arm instrumented with a non-invasive beat-to-beat blood pressure device for beat-to-beat arterial blood pressure measurement, and a brachial artery blood pressure cuff for calibration and verification of the beat-to-beat system. (C) Instrumentation of the non-dominant arm. The hand is comfortably gripping a handgrip dynamometer (connected to data acquisition system), and the forearm muscle is instrumented with the near-infrared spectroscopy probe. (D) Once instrumented, the NIRS optodes are covered with a black vinyl cloth (to eliminate interference from ambient light). In addition, a rapid cuff inflation system is placed over the brachial artery. Please click here to view a larger version of this figure.

Figure 2
Figure 2. Skeletal muscle oxidative capacity protocol. (A) Raw data tracing from a representative subject measured via NIRS, showing tissue saturation (StO2) over time. After establishing a stable baseline, the brachial artery of the non-dominant arm is occluded for five min in order to establish the subject's desaturation reserve (difference between baseline StOand the nadir). After recovery from the occlusion, the subject is instructed to perform a 50% isometric handgrip, followed by 18 rapid cuff inflation series to assess muscle oxygen consumption recovery kinetics. (B) Data analysis is then performed offline by calculating the average slope of each cuff occlusion series following exercise; illustrated here using hypothetical cuff occlusion series data. (C) In order to calculate the recovery time constant of muscle oxygenation, the slope of each of the 18 rapid cuff occlusions (i.e., post-exercise muscle oxygen consumption, mV̇O2) from A is plotted against time and fit to a monoexponential curve. Please click here to view a larger version of this figure.

Figure 3
Figure 3. Reactive hyperemia experimental protocol. With the subject lying supine, record at least 1 min of baseline data, followed by 5 min of total arterial cuff occlusion, and at least 3 min of recovery following cuff release. Note the obvious overlap between the skeletal muscle oxidative capacity protocol (Figure 2) and this protocol. 'Baseline' defines the period of time prior to arterial cuff occlusion. 'Slope 1' defines the desaturation rate during cuff occlusion, and is regarded as a measure of resting skeletal muscle metabolic rate. The lowest StO2 value obtained during ischemia is defined as 'StO2 minimum', and is regarded as a measure of the ischemic stimulus to vasodilate. The tissue saturation reperfusion rate is denoted as 'Slope 2', and is an index of reactive hyperemia; as are StO2 maximum, and the reactive hyperemia 'area under the curve' (AUC). To gain insight into the hyperemic reserve, the StO2 maximum is expressed as a percent change from baseline. Please click here to view a larger version of this figure.

Figure 4
Figure 4. Functional sympatholysis experimental protocol. Left panel: Raw data tracing from a representative subject. With the subject lying supine in the LBNP chamber, allow 3 min of steady-state baseline data collection. Turn on LBNP to -20 mmHg for 2 min. Oxyhemoglobin/myoglobin should decrease in response to the reflex sympathetic vasoconstriction (blue circle, shaded area). Allow 2 min for recovery. Ask the subject to perform rhythmic handgrip exercise at 20% MVC (measured prior to data collection). After 3 min of rhythmic exercise, repeat -20 mmHg LBNP for 2 min while the subject continues to exercise, followed by 2 min of exercise without LBNP. The reduction in oxyhemoglobin/myoglobin should be significantly attenuated (red circle, shaded area). If not already performed, inflate a blood pressure cuff over the brachial artery of the exercising arm for 5 min to establish the subject's range of desaturation. Note that the shaded areas in the figure are only meant to highlight the changes in oxyhemoglobin/myoglobin; see protocol for details on how to analyze the outcome variables used to calculate sympatholysis. Right Panel: LBNP-induced change in oxyhemoglobin/myoglobin at rest and during handgrip exercise calculated from the data on the left. Please click here to view a larger version of this figure.

Reference/Data Set  Study Population Sample size
Age of participants
(years ± SD)
Tau (τ)
Muscle group NIRS Variable reported Device
Brizendine et al. (2013) Endurance Athletes 8 25 ± 3 19 Vastus lateralis Hbdiff/total blood volume Continuous wave
(Oxymon MK III)
Ryan et al. (2014) Young, healthy 21 26 ± 2 55 Vastus lateralis HHb Continuous wave
(Oxymon MK III)
Southern et al. (2015) Elderly 23 61 ± 5 63 Wrist flexor Hbdiff Continuous wave
(Oxymon MK III)
Elderly + Heart Failure 16 65 ± 7 77 Wrist flexor Continuous wave
(Oxymon MK III)
Adami et al. (2017) Smokers with normal spirometry 23 63 ± 7 80 Medial forearm Tissue saturation index (TSI) Continuous wave
COPD Gold 2-4 16 64 ± 9 100 Medial forearm Continuous wave
Erickson et al. (2013) Spinal cord injury 9 43 ± 11 143 Vastus lateralis HbO2  Continuous wave
(Oxymon MK III)

Table 1: Summary of previously published reports across the health continuum using near-infrared spectroscopy to measure skeletal muscle oxidative capacity.

Reference Study Population Muscle Group Reported  Outcomes Outcome Value
Lacroix, J Biomed Opt, 2012 Healthy Males Forearm Peak Oxyhemoglobin 28.05 ± 3.15 μM
Peak Total Hemoglobin 10.56 ± 1.80 μM
Increase Rate to Peak HbO2 0.75 ± 0.22 μM/s
Increase Rate to Peak Total Hb 0.52 ± 0.16 μM/s
Kragelj, Ann Biomed Eng, 2001 Peripheral Vascular Disease Forearm Oxygen Consumption 0.68 ± 0.04 mL/min
Time to Peak 153 ± 16 s
Maximal Absolute Change in HbO2 2.93 ± 0.22 μM/100 mL
Suffoletto, Resuscitation, 2012 Post-Cardiac Arrest ICU Admittants Thenar Eminence Desaturation Rate -5.6 ± 2 %/min
Resaturation Rate 0.9 ± 0.6 %/sec
Dimopoulos, Respir Care, 2013 Pulmonary Artery Hypertension Thenar Eminence Baseline Saturation with 21% O2 65.8 ± 14.9 %
O2 Consumption Rate with 21% O2 35.3 ± 9.1 %/min
Reperfusion Rate with 21% O2 535 ± 179 %/min
Doerschug, Am J Physiol Heart Circ Physiol, 2007 Organ Failure  & Sepsis Forearm Baseline Saturation 84%
Reoxygenation Rate 3.6 %/s
Mayeur, Crit Care Med, 2011 Septic Shock Thenar Eminence Baseline Saturation 80 ± 1.0 %
Desaturation Slope -9.8 ± 3.7 %/min
Recovery Slope 2.3 ± 1.4 %/sec
McLay, Exp Physiol, 2016 Healthy Males Tibialis Anterior Baseline Saturation 71.3 ± 2.9 %
Minimum Saturation 44.8 ± 8.6 %
Desaturation Slope -0.1 ± 0.03 %/s
Recovery Slope 1.63 ± 0.5 %/s
Peak Saturation 82.6 ± 2.3 %
McLay, Physiol Rep, 2016 Healthy Males Tibialis Anterior Baseline Saturation 71.1 ± 2.4 %
Minimum Saturation 46.2 ± 7.5 %
Peak Saturation 82.1 ± 1.4 %
Recovery Slope 1.32 ± 0.38 %/s

Table 2: Summary of previously published reports across the health continuum using near-infrared spectroscopy to measure reactive hyperemia.

Reference Study Population % Attenuation
Nelson MD, J. Physiol, 2015 Healthy -57
Becker Muscular Dystrophy -13
Vongpatanasin, J. Physiol, 2011 Healthy -93
Hypertension -14
Fadel, J. Physiol, 2004 Pre-Menopause -84
Post-Menopause -19
Sander, PNAS, 2000 Healthy -74
Duchenne Muscular Dystrophy .+7
Nelson MD, Neurology, 2014 Healthy -54
Duchenne Muscular Dystrophy -7
Price, Hypertension, 2013 Hypertension Pre-Treatment -52
Hypertension Post-Nebivolol Treatment -97
Hansen, J. Clin. Invest., 1996 Healthy Exercise at 20% MVC -92
Healthy Exercise at 30% MVC -125

Table 3: Summary of previously published reports across the health continuum using near-infrared spectroscopy, in combination with lower body negative pressure and handgrip exercise, to assess functional sympatholysis.

Subscription Required. Please recommend JoVE to your librarian.


The methods described herein enable non-invasive, clinical evaluation of reactive hyperemia, neurovascular coupling, and skeletal muscle oxidative capacity in a single clinic or laboratory visit.

Critical Considerations

Although NIRS is relatively robust and easy to use, collection of these data require careful placement of the optodes directly over the muscle belly, secured tightly in place to avoid movement artifact, and covered with a black vinyl sheet in a dimly lit room to avoid interference of the near infrared from external light. In addition, obtaining good quality data relies heavily on clear communication between the tester and the subject, and the testing team. We, and others, have found that when performed with appropriate care and attention, NIRS is highly reproducible within a single study visit, and across multiple visits10,11,24,29. Moreover, the physiological outcome variables reported herein (i.e., skeletal muscle oxidative capacity, reactive hyperemia, and neurovascular coupling) are sensitive to experimental/clinical intervention, both within and between study visits30,31,10,11.

There is currently limited consensus on the appropriate reporting of the NIRS outcome variables. For example, when measuring skeletal muscle oxidative capacity, investigators have fit the recovery kinetics of HbO232, HHb19, Hbdiff30 and tissue Osaturation (present study and others33). Likewise, a similar spread in the outcome variables have also been reported for NIRS-based reactive hyperemia.34,35,36,37Some of this discrepancy may relate to the type of NIRS device used. For example, frequency-domain devices (as used here) provide absolute quantification of HbOand HHb, and thus may not be affected by acute changes in total Hb content (negating the need to correct the data). In contrast however, continuous-wave devices are greatly affected by acute changes in total hemoglobin, requiring data correction25.

Modifications and troubleshooting

One important and currently unavoidable limitation of NIRS is its limited penetration depth (~2 cm). Therefore, limb adiposity can significantly reduce — and even completely eliminate — the NIRS signal and should be considered when screening potential subjects. To control for this, investigators are encouraged to measure forearm skinfold thickness, and exclude participants with significant peripheral adiposity.

Any factor that can modulate vascular responsiveness, neurovascular coupling, and/or skeletal muscle oxidative capacity (i.e., medication, genetic mutations, etc.) will indeed affect the primary end-point measurements described herein. Investigators are therefore encouraged to take these factors into account when adapting this protocol and planning future experimentation.

For functional sympatholysis determination, investigators may wish to include a second resting LBNP challenge to ensure the signal is still present and that the differences observed during exercise-LBNP were not simply due to a loss of signal or measurement error. It is recommended to allow 3 - 5 min to allow the oxyhemoglobin signal to full recovery to baseline values before repeating the resting LBNP challenge.

Future applications or directions after mastering this technique

NIR spectroscopy uses laser light to assess the concentration of oxygenated and deoxygenated hemoglobin in tissue. During measurement of reactive hyperemia and functional sympatholysis, relative changes in these parameters are believed to represent changes in microvascular flow. Diffuse correlation spectroscopy (DCS) is an emerging near-infrared imaging approach which, in addition to evaluating the concentration of oxy- and deoxyhemoglobin, can also quantify microvascular perfusion38. Given the obvious similarities between these two imaging approaches, incorporation of DCS into the proposed techniques would be virtually seamless and may provide additional insight into the quantification of microvascular function and perfusion.

Once this technique is mastered, application to clinical populations, such as those with heart failure, will provide important mechanistic insight into exercise intolerance and cardiovascular dysfunction.

Subscription Required. Please recommend JoVE to your librarian.


The authors declare that they have no competing financial interests.


This work was supported by a University of Texas at Arlington Interdisciplinary Research Program grant.


Name Company Catalog Number Comments
Dual-channel OxiplexTS Near-infrared spectroscopy machine Iss Medical 101
NIRS muscle sensor Iss Medical 201.2
E20 Rapid cuff inflation system Hokanson E20
AG101 Air Source Hokanson AG101
Smedley Handgrip dynometer (recording) Stolting 56380
Powerlab 16/35, 16 Channel Recorder ADInstruments PL3516
Human NIBP Set ADInstruments ML282-SM
Bio Amp ADInstruments FE132
Quad Bridge Amp ADInstruments FE224
Connex Spot Monitor Welch Allyn 71WX-B
Origin(Pro) graphing software OrignPro Pro
Lower body negative pressure chamber Physiology Research Instruments standard unit



  1. Huang, A. L., et al. Predictive value of reactive hyperemia for cardiovascular events in patients with peripheral arterial disease undergoing vascular surgery. Arterioscler Thromb Vasc Biol. 27, (10), 2113-2119 (2007).
  2. Suryapranata, H., et al. Predictive value of reactive hyperemic response on reperfusion on recovery of regional myocardial function after coronary angioplasty in acute myocardial infarction. Circulation. 89, (3), 1109-1117 (1994).
  3. Richardson, R. S., et al. High Muscle Blood-Flow in Man - Is Maximal O2 Extraction Compromised. J of Appl Physiol. 75, (4), 1911-1916 (1993).
  4. Clifford, P. S., Hellsten, Y. Vasodilatory mechanisms in contracting skeletal muscle. J Appl Physiol. 97, (1), 393-403 (2004).
  5. Hansen, J., Thomas, G. D., Jacobsen, T. N., Victor, R. G. Muscle metaboreflex triggers parallel sympathetic activation in exercising and resting human skeletal muscle. Am J Physiol. 266, (6 Pt 2), H2508-H2514 (1994).
  6. Thomas, G. D., Victor, R. G. Nitric oxide mediates contraction-induced attenuation of sympathetic vasoconstriction in rat skeletal muscle. J Physiol. 506, (Pt 3), 817-826 (1998).
  7. Hansen, J., Thomas, G. D., Harris, S. A., Parsons, W. J., Victor, R. G. Differential sympathetic neural control of oxygenation in resting and exercising human skeletal muscle. J Clin Invest. 98, (2), 584-596 (1996).
  8. Rosenmeier, J. B., Fritzlar, S. J., Dinenno, F. A., Joyner, M. J. Exogenous NO administration and alpha-adrenergic vasoconstriction in human limbs. J Appl Physiol. 95, (6), 2370-2374 (2003).
  9. Fadel, P. J., Keller, D. M., Watanabe, H., Raven, P. B., Thomas, G. D. Noninvasive assessment of sympathetic vasoconstriction in human and rodent skeletal muscle using near-infrared spectroscopy and Doppler ultrasound. J Appl Physiol. 96, (4), 1323-1330 (2004).
  10. Nelson, M. D., et al. PDE5 inhibition alleviates functional muscle ischemia in boys with Duchenne muscular dystrophy. Neurology. 82, (23), 2085-2091 (2014).
  11. Nelson, M. D., et al. Sodium nitrate alleviates functional muscle ischaemia in patients with Becker muscular dystrophy. J Physiol. 593, (23), 5183-5200 (2015).
  12. Remensnyder, J. P., Mitchell, J. H., Sarnoff, S. J. Functional sympatholysis during muscular activity. Observations on influence of carotid sinus on oxygen uptake. Circ Res. 11, 370-380 (1962).
  13. Kodama, S., et al. Cardiorespiratory fitness as a quantitative predictor of all-cause mortality and cardiovascular events in healthy men and women: A meta-analysis. JAMA. 301, (19), 2024-2035 (2009).
  14. Westerblad, H., Place, N., Yamada, T. Muscle Biophysics: From Molecules to Cells. Rassier, D. E. Springer. New York. 279-296 (2010).
  15. Tyni-Lenné, R., Gordon, A., Jansson, E., Bermann, G., Sylvén, C. Skeletal muscle endurance training improves peripheral oxidative capacity, exercise tolerance, and health-related quality of life in women with chronic congestive heart failure secondary to either ischemic cardiomyopathy or idiopathic dilated cardiomyopathy. Am J of Cardiol. 80, (8), 1025-1029 (1997).
  16. Cabalzar, A. L., et al. Muscle function and quality of life in the Crohn's disease. Fisioter Mov. 30, 337-345 (2017).
  17. Esch, B. T., Scott, J. M., Warburton, D. E. Construction of a lower body negative pressure chamber. Adv Physiol Educ. 31, (1), 76-81 (2007).
  18. Ryan, T. E., Southern, W. M., Reynolds, M. A., McCully, K. K. A cross-validation of near-infrared spectroscopy measurements of skeletal muscle oxidative capacity with phosphorus magnetic resonance spectroscopy. J Appl Physiol. 115, (12), 1757-1766 (2013).
  19. Ryan, T. E., Brophy, P., Lin, C. T., Hickner, R. C., Neufer, P. D. Assessment of in vivo skeletal muscle mitochondrial respiratory capacity in humans by near-infrared spectroscopy: a comparison with in situ measurements. J Physiol. 592, (15), 3231-3241 (2014).
  20. Adami, A., Rossiter, H. B. Principles, insights and potential pitfalls of the non-invasive determination of muscle oxidative capacity by near-infrared spectroscopy. J Appl Physiol. (2017).
  21. Corretti, M. C., et al. Guidelines for the ultrasound assessment of endothelial-dependent flow-mediated vasodilation of the brachial artery - A report of the International Brachial Artery Reactivity Task Force. J Am Coll Cardiol. 39, (2), 257-265 (2002).
  22. Thijssen, D. H., et al. Assessment of flow-mediated dilation in humans: a methodological and physiological guideline. Am J Physiol Heart Circ Physiol. 300, (1), H2-H12 (2011).
  23. Green, D. J., Jones, H., Thijssen, D., Cable, N. T., Atkinson, G. Flow-mediated dilation and cardiovascular event prediction: does nitric oxide matter? Hypertension. 57, (3), 363-369 (2011).
  24. Southern, W. M., Ryan, T. E., Reynolds, M. A., McCully, K. Reproducibility of near-infrared spectroscopy measurements of oxidative function and postexercise recovery kinetics in the medial gastrocnemius muscle. Appl Physiol Nutr Metab. 39, (5), 521-529 (2014).
  25. Ryan, T. E., Erickson, M. L., Brizendine, J. T., Young, H. J., McCully, K. K. Noninvasive evaluation of skeletal muscle mitochondrial capacity with near-infrared spectroscopy: correcting for blood volume changes. J Appl Physiol. 113, (2), 175-183 (2012).
  26. Ryan, T. E., et al. Skeletal muscle oxidative capacity in amyotrophic lateral sclerosis. Muscle Nerve. 50, (5), 767-774 (2014).
  27. Mayeur, C., Campard, S., Richard, C., Teboul, J. L. Comparison of four different vascular occlusion tests for assessing reactive hyperemia using near-infrared spectroscopy. Crit Care Med. 39, (4), 695-701 (2011).
  28. McLay, K. M., et al. Vascular responsiveness determined by near-infrared spectroscopy measures of oxygen saturation. Exp Physiol. 101, (1), 34-40 (2016).
  29. McLay, K. M., Nederveen, J. P., Pogliaghi, S., Paterson, D. H., Murias, J. M. Repeatability of vascular responsiveness measures derived from near-infrared spectroscopy. Physiol Rep. 4, (9), (2016).
  30. Ryan, T. E., Southern, W. M., Brizendine, J. T., McCully, K. K. Activity-induced changes in skeletal muscle metabolism measured with optical spectroscopy. Med Sci Sports Exerc. 45, (12), 2346-2352 (2013).
  31. Southern, W. M., et al. Reduced skeletal muscle oxidative capacity and impaired training adaptations in heart failure. Physiol Rep. 3, (4), (2015).
  32. Ryan, T. E., Brizendine, J. T., McCully, K. K. A comparison of exercise type and intensity on the noninvasive assessment of skeletal muscle mitochondrial function using near-infrared spectroscopy. J Appl Physiol. 114, (2), 230-237 (2013).
  33. Adami, A., Cao, R., Porszasz, J., Casaburi, R., Rossiter, H. B. Reproducibility of NIRS assessment of muscle oxidative capacity in smokers with and without COPD. Respir Physiol Neurobiol. 235, 18-26 (2017).
  34. Lacroix, S., et al. Reproducibility of near-infrared spectroscopy parameters measured during brachial artery occlusion and reactive hyperemia in healthy men. J Biomed Opt. 17, (7), 077010 (2012).
  35. Bopp, C. M., Townsend, D. K., Warren, S., Barstow, T. J. Relationship between brachial artery blood flow and total [hemoglobin+myoglobin] during post-occlusive reactive hyperemia. Microvasc Res. 91, 37-43 (2014).
  36. Willingham, T. B., Southern, W. M., McCully, K. K. Measuring reactive hyperemia in the lower limb using near-infrared spectroscopy. J Biomed Opt. 21, (9), 091302 (2016).
  37. Kragelj, R., Jarm, T., Erjavec, T., Presern-Strukelj, M., Miklavcic, D. Parameters of postocclusive reactive hyperemia measured by near infrared spectroscopy in patients with peripheral vascular disease and in healthy volunteers. Ann Biomed Eng. 29, (4), 311-320 (2001).
  38. Gurley, K., Shang, Y., Yu, G. Noninvasive optical quantification of absolute blood flow, blood oxygenation, and oxygen consumption rate in exercising skeletal muscle. J Biomed Opt. 17, (7), 075010 (2012).



    Post a Question / Comment / Request

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

    Usage Statistics