Quantification of Neurovascular Protection Following Repetitive Hypoxic Preconditioning and Transient Middle Cerebral Artery Occlusion in Mice

Summary

This protocol describes repetitive hypoxic preconditioning, or brief exposures to systemic hypoxia that reduce infarct volumes and blood-brain barrier disruption following transient middle cerebral artery occlusion in mice. It also details dual quantification of infarct volume and blood-brain barrier disruption after stroke to assess the efficacy of neurovascular protection.

Abstract

Experimental animal models of stroke are invaluable tools for understanding stroke pathology and developing more effective treatment strategies. A 2 week protocol for repetitive hypoxic preconditioning (RHP) induces long-term protection against central nervous system (CNS) injury in a mouse model of focal ischemic stroke. RHP consists of 9 stochastic exposures to hypoxia that vary in both duration (2 or 4 hr) and intensity (8% and 11% O₂). RHP reduces infarct volumes, blood-brain barrier (BBB) disruption, and the post-stroke inflammatory response for weeks following the last exposure to hypoxia, suggesting a long-term induction of an endogenous CNS-protective phenotype. The methodology for the dual quantification of infarct volume and BBB disruption is effective in assessing neurovascular protection in mice with RHP or other putative neuroprotectants. Adult male Swiss Webster mice were preconditioned by RHP or duration-equivalent exposures to 21% O₂ (i.e. room air). A 60 min transient middle cerebral artery occlusion (tMCAo) was induced 2 weeks following the last hypoxic exposure. Both the occlusion and reperfusion were confirmed by transcranial laser Doppler flowmetry. Twenty-two hr after reperfusion, Evans Blue (EB) was intravenously administered through a tail vein injection. 2 hr later, animals were sacrificed by isoflurane overdose and brain sections were stained with 2,3,5- triphenyltetrazolium chloride (TTC). Infarcts volumes were then quantified. Next, EB was extracted from the tissue over 48 hr to determine BBB disruption after tMCAo. In summary, RHP is a simple protocol that can be replicated, with minimal cost, to induce long-term endogenous neurovascular protection from stroke injury in mice, with the translational potential for other CNS-based and systemic pro-inflammatory disease states.

Introduction

As the leading cause of adult disability and the fourth leading cause of death, stroke is one of the most debilitating disease states facing the adult population of the United States.¹ Animal models of stroke allow for experimental investigation of new methods of reducing ischemic injury and improving post-stroke recovery. One novel avenue for such translational research is preconditioning. Preconditioning is the intentional use of a non-damaging stimulus to reduce damage from a subsequent, and more severe, injury.² Hypoxic preconditioning has been shown to produce pleiotropic changes in the brain that provide protection against stroke in both in vivo and in vitro studies.³ However, a single exposure to hypoxia only offers short-term neuroprotection, inducing less than 72 hr of tolerance against ischemia in adult mice.⁴ Even after four weeks of 14 hr daily exposures to hypobaric hypoxia, Lin et al. found that neuroprotection was only sustained for one week.⁵ Repetitive hypoxic preconditioning (RHP) is characterized by stochastic variations in frequency, duration, and intensity of hypoxic exposures. In contrast to a single preconditioning challenge, RHP induces a cerebroprotective phenotype that lasts up to eight weeks in mice.⁶ RHP reduced infarct volumes, blood-brain barrier (BBB) disruption, vascular inflammation, and leukocyte diapedesis for weeks after the final hypoxic exposure. RHP specifically reduced inflammation in the ischemic brain by reducing T cell, monocyte, and macrophage populations, while maintaining B cell populations in the ischemic hemisphere.⁷ In fact, RHP induced an immunosuppressive phenotype in mice prior to any CNS injury, including stroke. RHP-treated B cells isolated from RHP-treated healthy mice exhibited a unique anti-inflammatory phenotype, with a downregulation of both antigen presentation and antibody production. The overall reduction in pro-inflammatory adaptive immune mechanisms makes RHP an excellent methodology to induce endogenous immunosuppression for not only CNS-specific inflammatory diseases, but also systemic injury or disease models that include a pro-inflammatory pathology.

RHP reduces both infarct volume and BBB disruption following a transient middle cerebral artery occlusion (tMCAo). Animal models of stroke, such as the commonly used tMCAo, dramatically improve the understanding of the pathophysiology of stroke, as well as the design of more effective neurotherapeutics. First developed by Koizumi et al., in 1986,⁸ the tMCAo procedure is a widely used method of inducing stroke in rodents and one of the preferred methods for investigating inflammation following reperfusion. As the methods for tMCAo evolve, the more recent use of silicone-coated filaments further reduce the risk of subarachnoid hemorrhage compared to other models^9,10 and improve reliability, though unfortunately tMCAo often produces a wide variation in infarct volumes.^11-13 Most of these studies delineate infarction regions in coronal brain sections by staining with 2,3,5- triphenyltetrazolium chloride (TTC), considered a gold standard for infarct quantification because it is a simple and inexpensive way to produce vivid, replicable results. TTC serves as a substrate of dehydrogenases present in mitochondria. When brain slices are exposed to the TTC solution, TTC is selectively taken into living cells where its non-soluble reduction product, formazan, precipitates to a deep red color in viable mitochondria. Because of mitochondrial dysfunction in the ischemic tissue, this tissue remains white, allowing for differentiation of damaged and healthy tissue.¹⁴

RHP also reduces BBB disruption in the ischemic hemisphere.⁶ Therefore, the dual quantification of BBB integrity within the same brains as TTC-based infarct volume determinations¹⁵ would provide useful information about the full efficacy of endogenous protection, and potential causal relations between BBB disruption and infarction in untreated and treated animals. The influx of peripheral blood through a disrupted BBB, secondary to stroke, increases leukocyte populations, pro-inflammatory cytokines, oxidative stress, vasogenic edema, and hemorrhagic transformation in the ischemic hemisphere, ultimately increasing the rates of infection and mortality in patients with ischemic stroke.^16,17 A common method of measuring BBB disruption in animal models is through quantification of Evans blue (EB) dye leak into the brain.^15,18-21 EB selectively binds to serum albumin, a globular protein (MW=65 kDa) that does not cross the BBB in uninjured animals.²² Following ischemic stroke, EB infiltrates the brain, and fluoresces at 620 nm, allowing for measurement of optical density within the perfused injured parenchyma.²² The optical density is directly proportional to the permeability of the BBB when EB has been washed out of the post-mortem cortical vasculature by transcardiac perfusion. With the immediate processing of TTC-stained brains in animals with EB administration, both the infarct volume and BBB disruption can be effectively quantified. It should be noted, however, that neuronal injury and BBB disruption are not concomitant processes in the post-stroke brain,^23,24 so the selection of time of sacrifice is an important consideration.

The protocol that follows details the RHP method, the tMCAo method for inducing a temporary arterial occlusion that models middle cerebral artery occlusions in human patients, and the dual histological methods for determining neural and vascular stroke injury endpoints. TTC measures cell death and cumulative tissue damage, allowing for the quantification of an overall infarct volume, while EB provides for the hemispheric quantification of BBB damage.

Protocol

NOTE: This protocol was approved by the Institutional Animal Care and Use Committee (IACUC) at UT Southwestern Medical Center which abides by the National Institutes for Health (NIH) policy for experimental animal usage.

1. Repetitive Hypoxic Preconditioning

1. Custom design four flowmeters on gas regulators and attach to standard 15 L induction chambers with PVC tubes to allow compressed gas from the oxygen (O₂) tanks to flow into the chambers via an inlet port. See Equipment and Materials for more details about custom design.
2. Divide mice into 2 groups: Repetitive Hypoxic Preconditioning (RHP) Group, which receive exposures to 8% and 11% O₂, and the Control Group, which receive exposures to 21% O₂ (room air) concurrently. See Table 1 for the variations in frequency, intensity (8 and 11% O₂ or 21% O₂), and duration (2 or 4 hr) of RHP exposures.
3. Remove the top filter lid of each cage and place the cage, with food and water bottles intact, in the chambers connected to their respective O₂ tanks. Close and secure the lid of the chamber.
   1. Open the main gas valve for the tanks and set the initial flow for each induction chamber to 2 L per min (LPM) for the first 5 mins of exposure. Reduce the flow rate to 1 LPM for the remainder of the exposure.
   2. At the end of the exposure, reduce the flow to to 0 LPM and close the gas valve for the tanks.
   3. Open the chamber lids and replace the filter top lid on each cage. Place the cages in standard housing until the next hypoxic exposure.
4. Spray down each induction chamber with NPD (Steris) or an equivalent disinfectant/deodorizer after each use.
5. Expose both 21% and RHP mice at the same time of day over the course of two weeks as described in Table 1.

2. Transient Middle Cerebral Artery Occlusion (tMCAo)

1. See Discussion for more details on the timing of stroke following final RHP exposure.
2. Prepare an aseptic surgery workplace. Clean surrounding workplace with 70% Ethanol or an equivalent disinfectant and autoclave all surgical tools.
   1. Set up the Laser Doppler Flowmetry (LDF) instrument to measure relative changes in cerebral blood flow (CBF). Turn on the heating pad to 37 °C. Turn on the incubator to 34 °C.
3. Anesthetize mice with a brief exposure to a mix of 4% isoflurane/70% NO₂/30% O₂ in a small induction chamber. Confirm proper anesthesia by lightly pinching the paw. If the mouse withdraws its paw, return the mouse to the induction chamber and continue isoflurane exposure.
4. Remove mice from the anesthesia induction chamber and quickly insert the mouse’s nose in the nose cone. Open the gas flow to the nose cone, closing off flow to the anesthesia induction chamber.
   1. Without changing the 70% NO₂/30% O₂ gas mixture, fix isoflurane at 1.8% as the maintenance dose for the remainder of the procedure. Breathing should remain slow and regular throughout the procedure but if breathing becomes rapid and shallow, increase the isoflurane dose. Maintenance dose may vary between equipment manufacture and animal used in the experiment.
5. Using a microshaver, shave the hair on the temporal region between the corner of the eye and the ear as well as ventral midline of the neck. Remove excess fur and apply ocular lubricant with a sterile cotton swab to keep the corneas from drying out during the procedure. Wipe down incision area with alcohol pads and swab providone-iodine with a sterile cotton swab to maintain aseptic conditions.
6. Administer analgesics according to rodent surgical guidelines.
7. Make an incision through the temporal skin between the eye and the ear. Expose the temporalis muscle. Using surgical micro-scissors, cut the temporal muscle ligament at the temporal ridge within the area of white muscle striation.
   1. Gently push the muscle bulk laterally with forceps to visualize the middle cerebral artery (MCA) through the skull. After incision of the temporal muscle, the area may fill with blood. Gently use a cotton swab to staunch any potential bleeding.
   2. Target the the LDF probe tip to the MCA area. Record the vessel chosen as this area varies between mice.
   3. Hold the LDF in place and flush with the skull until a stable red blood cell flux is read and record this value as the baseline CBF. Ideal baseline CBF on a Laser Doppler Flowmetry are >600 flux, but this will vary with manufacturer. If baseline CBF is <400 flux, the flow recording is most likely from a nearby vein, or an incomplete placement of the probe over the target vessel.
8. After baseline CBF is established, reposition the mouse so that the neck is exposed. Support its head and keep the mouse under steady anesthesia from the nosecone.
9. Make a ventral midline incision from just below the mandible to the clavicle.
   1. Using forceps, blunt dissect all superficial fascia to expose the left common carotid artery (CCA). Separate the CCA from connective tissue and the vagus nerve.
   2. Permanently ligate the CCA with a 6.0 silk suture. Place the ligating suture as proximal as possible to allow enough room for occluding filament placement.
   3. Loop and loosely tie a second silk 6.0 suture around the CCA distal to the occluding suture. Be careful not to occlude the artery as the occluding filament will subsequently be threaded through the carotid.
   4. Use an 8 x 2 mm light micro serrafine areterial clamp to clamp the CCA distal to the loosely-tied silk suture. Gently lift the CCA with forceps and make a small longitudinal incision, as proximal to the ligating suture as possible with 3 mm vannas.
   5. Thread a 12 mm silicon-coated 6.0 gauge nylon occluding filament through the incision to enter the artery lumen, and then advance it a few mm. Loosely tighten the second loose silk suture around the tip of the occluding filament to ensure blood flow does not push the filament out of the CCA and remove the arterial clamp.
   6. At the first bifurcation of the CCA into the internal carotid artery (ICA) and the external carotid artery (ECA), thread the occluding filament into the right branch of the first bifurcation to enter the ICA.Advance the occluding filament 9 to 10.5 mm past the second silk suture into the left internal carotid artery (ICA).
   7. Shortly after entering the ICA, advance the occluding filament into the left branch at the second bifurcation between the ICA and the pterogopalantine artery (PPA). Visualization of the PPA is unlikely so proceed until you feel a mild resistance with full placement of the occluding filament. Lifting the ICA with forceps may help the filament to thread more easily into the left branch of the second birfurcation. Tighten the second silk suture.
   8. Turn the mouse so the incision over the MCA is visible. With the LDF equipment, confirm that the CBF is blocked through LDF readings. A successful occlusion is a >80% reduction from baseline CBF.
   9. Completely tighten and double-knot the second silk suture around the occluding filament when the proper position is achieved. If necessary, slightly push in or pull out the occluding filament to achieve CBF criteria for a successful occlusion (e.g. >80% reduction from baseline CBF).
   10. Close the neck and head opening with 6.0 nylon sutures.
10. Place mice in the 34 °C incubator for the duration of the occlusion. Recommended length of occlusion is 60 min, but this varies for age, strain-dependent differences in cerebrovascular anatomy,²⁵ and the extent of injury desired (mild, moderate, severe). Make sure that animals regain consciousness within mins of coming off anesthesia.
11. Re-anesthetize the animals with isoflurane, as described in step 2.3, 5 min before the end of the pre-defined occlusion period, open the scalp incision and confirm that the MCA perfusion is still reduced using transcranial LDF readings. If CBF is not sufficiently reduced (e.g. <20% baseline CBF), the MCA has reperfused at some point during the occlusion and the mouse should be excluded from further experimentation.
12. Open the midline neck incision and loosely tie a third silk suture around the CCA, distal to the second silk suture but proximal to the CCA bifurcation to ensure that the external carotid artery (ECA) will remain viable after the filament is removed.
    1. Cut or untie the knot that holds the occluding filament (i.e., second silk suture) and withdraw the occluding filament slowly. Once removed, quickly close the third silk suture around the CCA to minimize backflow of blood from the ICA. Double-knot this suture and close the incision with 6.0 nylon sutures.
    2. Reposition the mouse to quantify the level of CBF after 5 min of reperfusion. Successful reperfusion is generally defined as a CBF of >50% of baseline CBF, but, as with occlusion flow, investigators can establish their own criterion. If animals exhibit a CBF below 50% of their baseline, it is likely the MCA is ‘permanently’ occluded, and thus represents another study exclusion criterion.
    3. Close both incisions with 6.0 nylon sutures. Provide saline, anesthetic (Lidocaine), and antibiotics according to rodent guidelines. However some small doses of antibiotics (3 mg/kg of minocycline) have been found to be neuroprotective following stroke.²⁶
13. After regaining consciousness in the heated incubator following surgery, place mice in a clean, sterile cage. Provide moistened food or nutritional hydration dietary gel supplements and a petri dish of water as the animals will have restricted mobility following stroke. Monitor animals closely during recovery for excessive post-surgical pain and death.

3. Evans Blue (EB) Injection

1. Inject EB 22 hr after reperfusion and should circulate in the bloodstream for 2 hr prior to sacrifice and TTC staining.
2. Make an EB solution for injection (2% EB in saline) and gently mix at room temperature. Filter solution through filter paper or push through a 0.2 µm filter attached to a small syringe to remove undissolved EB and store at room temperature.
3. Prepare the amount of EB needed for injection (4 ml/kg of body weight) Draw the desired amount of dye into a 0.3 cc insulin syringe with a 29 gauge needle and ensure that the solution is at room temperature
   1. Restrain mouse using flat bottom restrainer. Hold the tail so that the lateral vein is uppermost. Lateral veins are located on either side of the centerline of the tail. Hold the tip of the tail to keep the mouse steady for injection.
   2. Insert the needle into the vein approximately 3.5 mm, being careful not to perforate the vein. Confirm that the needle is in the vein by drawing back on the syringe and looking for traces of blood.
   3. Inject all of the dye over the course of 1 min. If the solution is going into the vein there should be minimal resistance as pressure is applied to the syringe. Confirm successful systemic venous administration of EB by an immediate color change in the tail, limbs, and eyes of the mouse.
   4. Remove the needle from the tail and gently apply pressure using clean gauze in order to stop bleeding.
4. Begin timing when the mouse’s skin turns blue. Allow the EB to circulate for 2 hr to penetrate the weakened BBB.

4. 2,3,5- Triphenyltetrazolium Chloride (TTC) Staining

1. Perfusion and TTC staining should occur 24 hr after reperfusion.
2. Prepare a 2% TTC solution prior to the designated time of sacrifice. Add 10 g of TTC powder to 500 ml of 0.01 M phosphate buffered saline (PBS), pH 7.4. Heat solution to 37 °C in water bath to facilitate solubilizing of the TTC. CAUTION: TTC powder and solution are a skin, lung, and eye irritant. Wear appropriate personal protective equipment when handling these materials.
   1. Once the powder has completely dissolved, immediately transfer to a bottle, cover in foil, and store at 4 °C. TTC and tissue stained with TTC are light sensitive.
3. At 24 hr after tMCAo and 2 hr after EB administration, sacrifice the animal with an isoflurane overdose in a small induction chamber. Perfusion should begin immediately following sacricice in order to minimize autolysis which begins in the absence of oxygen following death.
4. Quickly secure the animal on a Styrofoam platform with forearms pinned through the paws. Cut a lateral incision through the abdominal wall from the midline just below the ribcage. Carefully cut through the diaphragm to expose the heart.
   1. Start the perfusion pump at 5 ml/min flow rate with a 60 cc syringe filled with ice cold 0.01 M PBS and connected to a 27 guage winged infusion needle. Place the tip of the needle about 0.5 cm into the left ventricle of the heart and cut the right atrium. Progressively diluted venous blood should flow out of the atrium during the perfusion until venous blood appears colorless. Transcardially perfuse 30 ml 0.01 M phosphate buffered saline (PBS) through the heart.
5. Add 5 ml of TTC solution into transparent 20 scintillation bottles.
6. Immediately following perfusion, decapitate the animals and dissect out the brains using small scissors and a spatula if necessary. Examine the brains to exclude animals which underwent subarachnoid hemorrhage at the Circle of Willis, secondary to suture placement. Check that the hemisphere contralateral to the occluded MCA appears pale, without noticeable EB leakage or edema.
7. Pour PBS into an acrylic brain matrix designed to make 1.0 mm thick coronal sections of a mouse brain. Place the brain, dorsal side up, into the matrix and immediately pour PBS over the brain. Keep the brain moist.
   1. Remove the olfactory bulbs by inserting a stainless steel 0.21 mm thick blade into the second slot from the rostral side of the matrix.
   2. Remove the cerebellum by inserting a blade in the fourth slot from the caudal side of the matrix.
   3. Insert a blade into the middle slot of the remaining slots in the matrix. Insert the remaining blades, evenly bisecting the remaining tissue to ensure the most even distribution of tissue during the slicing.
   4. Once all blades have been inserted, add 1 to 2 drops of PBS to the brain to moisten it.
   5. Remove the blades one at a time from the matrix beginning with the rostral region. Keep the first 7 slices for TTC analysis after tMCAo. Use a small spatula to carefully transfer the slices from the blade to the TTC-filled vial.
8. After all sections are in the vial, cap it and place in a warm water bath until the sections turn pink. Gently turn the bottle in the bath if necessary to avoid section overlap, which could lead to uneven staining. Then dispose of the TTC and pour a 4% paraformaldehyde solution into the vial to cover brain sections to terminate the TTC chemical reaction.
9. Immediately arrange the sections on a clean 1" x 3” glass slide and orient the sections from rostral to caudal.
   1. When the sections are arranged on the slide, scan the slide using a standard scanner. Set the resolution at a minimum of 600 dpi for image analysis. Be sure to include the name of the animal and a metric ruler in the scanned image.
   2. Flip over the slide and scan the back side to ensure all data is collected.

5. Infarct Volume Quantification

1. Quantify the infarct volume by using a standard image analysis software (e.g., ImageJ).
2. Scan images at a high resolution (e.g. 600 dpi) for adequate analysis. Crop images. Standardize the scale for all images using the metric ruler included in the scanned image.
3. Calculate the total volume of the contralateral hemisphere using the following formula. Repeat this formula to calculate the total volume of the ipsilateral hemisphere.
   Sum of total contralateral hemisphere of each slice x slice thickness
4. Calculate the indirect infarct volume. Control for ipsilateral edema from stroke by using the healthy, contralateral hemisphere as a control.²⁷ Use the following formula to calculate the indirect infarct volume:
   Total volume of contralateral hemisphere -
   (Total volume of ipsilateral hemisphere –Average volume of 3 measurements of infarct)

6. Blood-brain Barrier (BBB) Integrity Quantification

1. To prepare for EB quantification, first weigh 2.5 inch weigh boats. Record the weight and label two weigh boats for each animal: one for the ipsilateral hemisphere and one for the contralateral hemisphere.
2. After scanning the TTC-stained sections, bisect each section with a disposable razor blade into ipsilateral and contralateral hemispheres. Place the ipsilateral hemispheres from all 7 sections in a weigh boat and record the weight. Repeat for contralateral hemisphere.
3. Immediately transfer the weight boats to an oven set for 56 °C for 48 hr.
4. Weigh the dried sections. Transfer both hemispheres into separate 1.5 ml microcentrifuge tubes.
   1. Calculate the amount of formamide needed for each hemisphere (8 ml/g of dry tissue), and add to their respective microcentrifuge tubes. Formamide is light sensitive and cover all formamide-treated samples in foil from this point onward.
   2. Transfer the microcentrifuge tubes to an incubator set to 56 °C for another 48 hr.
5. After the 48 hr, pipette out the blue supernatant into another set of labeled microcentrifuge tubes. Push tissue to the bottom of the tube to maximize the volume of extracted supernatant. Keep the tubes of supernatant and dispose of all tissue.
6. Prepare exponential serial dilutions of EB in formamide for the standard curve. Include 1 blank (formamide only) and then 10 exponential solutions from 0.125 ug/ml through 64 ug/ml of EB in formamide.
   1. Pipette 300 µl of the dilutions made for the standard curve into a 96-well plate. Pipette 300 µl of the supernatant into corresponding wells.
   2. Measure the absorbance on a spectrophotometer at 620 nm.
   3. Compare the standard curve of the EB dilutions with the absorbance of the supernatant samples. The optical density is directly proportional to the integrity of the BBB.
   4. Assume the optical density of the contralateral hemisphere as background and use the formula (ipsilateral-contralateral)/contralateral to determine fold change. For further details about statistical analysis see Martin et al., 2010.¹⁸

Results

This study included 25 male Swiss Webster mice that were 10 weeks of age at the start of randomization into RHP (n = 10) or 21% O₂ (n = 15) groups. Two weeks after the final RHP exposure, surgical procedures were performed, with groups blinded and counterbalanced between days. Following tMCAo, 1 mouse died during post-operative recovery and 1 mouse was excluded from the study because it did not meet the reperfusion CBF criterion. Both excluded mice were from the 21% O₂ group. In accordance with ARRI...

Discussion

A single exposure to systemic hypoxia (i.e., 2 hr of 11% O₂) in mice “transiently” protects the brain from tMCAo,²⁹ meaning the epigenetic response to the hypoxic preconditioning challenge is short-lasting, and the baseline phenotype is restored within days. Repetitive presentations of the hypoxic preconditioning stimulus dramatically extend the duration of the neuroprotective phenotype.⁶ Many studies have shown that the frequency, magnitude, and duration of the repet...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
Flowmeters, regulators	VetEquip, Inc	Specialty order	Four flowmeters are attached to 6.0 mm flexible PVC tubing which connects to the inlet port on each induction chamber with a plastic female connector. These flowmeters are bolted to a 6.5" x 1" x 1" metal bar. This metal bar is bolted to a MI-246-P pressure gauge with a DISS outlet. This pressure gauge and flowmeter equipment can be attached to each new gas cylinder with a wrench.
21% O2 tank	AirGas	OX USP200
11% O2 tank	AirGas	Specialty order
8% O2 tank	AirGas	Specialty order
15 L induction chambers	VetEquip	941454
Moor Laber Dopper Flow	Moor Instruments	moorVMS-LDF1-HP	0.8 mm diameter probe
High Intensity Illuminator	Nikon	NI-150
Zoom Stereo Microscope	NIkon	SMZ800	Other surgical microscopes may be used.
Kent Scientific Right Temperature CODA	Kent Scientific Corporation	Discontinued	Recommended replacement is PhysioSuite with RightTemp Temperature Monitoring and Homeothermic Control (Kent Scientific, #PS-RT).
Hovabator Incubator	Stromberg's	2362-E	Our model is the 2362N. 2362E is a later model and includes an electronic thermostat.
V010 Anesthesia system	VetEquip	901807	Includes: ten foot high-pressure oxygen hose, frame, flowmeter, oxygen flush assembly, vaporizer, breathing circuit, chamber, nosecones, waste gas evacuation tubing and two VapoGuard filters
250 ml isoflurane	Butler Schein	NDC-11695
D-6 Vet Trim Animal Cordless Trimmer	Andis	#23905	Replacement blades are available from Andis (#23995)
Betadine	Fisher Scientific	19-898-867
Q-tips	Multiple sellers	Catalog number not available
Gauze Pads	Fisher Scientific	67622
Surgical drape	Fisher Scientific	GM300
Silk Sutures	Look/Div Surgical Specialties	SP115
Nylon Sutures	Look/Div Surgical Specialties	SP185
Durmont #5 forceps (2)	Fine Science Tools	11251-35	Angled 45°
Surgical Scissors	Fine Science Tools	14028-10
3 mm Vannas	Kent Scientific Corporation	INS600177	Straight blade
Hartman Hemostats	Fine Scientific Tools	13002-10
Occluding filaments	Washington University	Specialty order	Filaments are silicone coated at Washington Univeristy and provided to UTSW facilities for a fee.
Evans Blue	Sigma Aldritch	E2129-10G
Filter Paper	Sigma Aldritch	WHA1001150	150 mm, circles, Grade 1
Weigh Boats	Fisher Scientific	02-202-101	2.5" diameter
0.9% Sodium Chloride Injection USP	Baxter Pharmaceutics	2B1321
0.3 cc insulin syringe with 29 gauge needle	Becton Dickinson Labware	309301
Flat bottom restrainer	Braintree Scientific	FB M	2.0" diameter
TTC	Sigma	T8877
10x PBS, pH 7.4	Fisher Scientific	BP399-20
Water Bath	Multiple sellers	Catalog number not available	Scintillation tubes with TTC may be manually held under running warm water as an alternative to the water bath.
Styrofoam board	Multiple sellers	Catalog number not available
Large Syringe Kit	PumpSystems Inc	P-SYRKIT-LG
Perfusion Pump	PumpSystems Inc	NE-300
60 cc syringe	Fisher Scientific	NC9203256
27 gauge winged infusion set	Kawasumi Laboratories, Inc	D3K1-25G 1
20 ml scintillation vial	Fisher Scientific	50-367-126
Stainless steel spatula	Fisher Scientific	14-373-25A
Alto acrylic 1.0 mm mouse brain, coronal	CellPoint Scientific	Catalog number not available
0.21 mm stainless steel blades, 25 pk	CellPoint Scientific	Catalog number not available	Reusable cryostat blades are an inexpensive alternative.
4% paraformaldehyde	Santa Cruz Biotechnology	SC-281692
Superfrost microscope slides	Fisher Scientific	12-550-15
HP Scanjet G4050	Multiple sellers	Catalog number not available	Other commercial scanners are suitable for this step in the protocol.
ImageJ	National Institute of Health	Catalog number not available
Analytical Balance	Mettler Toledo	XSE 205U
Precision Compact Oven	Thermo Scientific	PR305225M
1.7 ml microcentrifuge tubes (Eppendorfs)	Denville Scientific	C2170
Formamide	Fisher Scientific	BP228-100
96-well plates	Fisher Scientific	07-200-9
Epoch Microplate Spectrophotometer	BioTek	Catalog number not available