Autoradiographic Measurements of [14C]-Iodoantipyrine in Rat Brain Following Central Post-Stroke Pain

Summary

We present a protocol to measure [¹⁴C]-iodoantipyrine (IAP) uptake and assess the activation of neural substrates that are involved in central post-stroke pain (CPSP) in a rodent model.

Abstract

Approximately 8% of stroke patients present symptoms of central post-stroke pain (CPSP). CPSP is associated with allodynia and hypersensitivity to nociceptive stimuli. Although some studies have shown that neuropathic pain may involve the dorsolateral prefrontal cortex, rostral anterior cingulate cortex, amygdala, hippocampus, periaqueductal gray, rostral ventromedial medulla, and medial thalamus, the neural substrates and their connections that mediate CPSP remain unclear. [¹⁴C]-Iodoantipyrine (IAP) uptake can be measured to evaluate spontaneously active pain. It can be used to assess the activation of neural substrates that may be involved in CPSP in an animal model. The [¹⁴C]-IAP method in rats is less expensive to perform compared with other brain mapping techniques. The present [¹⁴C]-IAP protocol is used to measure the activation of neural substrates that are involved in CPSP that is induced by lesions of the ventral basal nucleus (VB) of the thalamus in a rodent model.

Introduction

Stroke hemorrhage has been shown to occur in more than 8% of patients who suffer from neuropathic pain, referred to as central post-stroke pain (CPSP).^1-3 CPSP can result from somatosensory dysfunction, thereby inducing hypersensitivity and allodynia.⁴ However, the pathophysiological mechanisms of somatosensory dysfunction in CPSP remain uncertain. For example, the loss of somatic sensations results from neuronal deafferentation in the hemorrhagic brain area. Hyperalgesia may be caused by the hyperexcitability of central nociceptive neurons or central disinhibition,^{5, 6} but the neural substrates that are involved in CPSP symptoms remain unknown. Some studies have suggested that the dorsolateral prefrontal cortex (dPFC), rostral anterior cingulate cortex (ACC), amygdala, hippocampus, periaqueductal gray (PAG), rostral ventromedial medulla, and their connections with each other mediate nociceptive processing.⁷ Additionally, medial prefrontal cortex (mPFC)-amygdala circuits were shown to be involved in pain-related perception.⁸ Data on the pathophysiological mechanisms of CPSP are diverse, and the activation of neural substrates in CPSP needs further scrutiny.

[¹⁴C]-Iodoantipyrine (IAP) uptake is used to indirectly observe regional cerebral blood flow (rCBF), assuming a relationship between brain activity and CBF. Although [¹⁴C]-IAP cannot assess brain activity in real time, such as with functional magnetic resonance imaging (fMRI), it has several advantages. For example, [¹⁴C]-IAP is suitable for measuring spontaneously occurring brain events during pathological states.⁹ Moreover, [¹⁴C]-IAP uptake is measured without anesthesia. It also costs less than other imaging methods, including fMRI and positron emission tomography (PET). The [¹⁴C]-IAP method has been suggested to be appropriate for measuring spontaneous pain (e.g., CPSP) that is induced by lesions of the ventral basal nucleus (VB) of the thalamus.⁹

The present protocol describes how to perform the [¹⁴C]-IAP method to assess the involvement of neural substrates of CPSP that is induced by lesions of the VB of the thalamus in an animal model. The technique offers a way of determining the pathophysiological mechanisms that underlie CPSP symptoms at the behavioral and neuronal levels.

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Protocol

The protocol in the present study received approval from the Academia Sinica Institutional Animal Care and Utilization Committee in Taiwan.

1. Animal Preparations

1. Obtain male Sprague-Dawley rats (approximately 300 - 400 g). Maintain the rats in an air-conditioned room (21 - 22 °C, 50% humidity) under a 12 hr/12 hr light/dark cycle (lights on at 8:00 AM) with free access to food and water.

2. Experimental Procedure

1. Allow all of the rats to adapt to the environment in their home cages for 1 week before the experiments. During adaptation, perform the von Frey and plantar tests to establish baselines.
2. von Frey Test
   1. Place the rat in an acrylic enclosure (30 cm × 30 cm × 80 cm) for 30 min for habitation.
   2. Obtain von Frey filaments (filament no. 11 - 20) that have the same length but varying diameters to provide a range of forces of 2 - 100 g.
   3. To assess the paw withdrawal threshold in the rat's hindpaw, use von Frey filaments to stimulate the center of the hindpaws through a net-like port on the acrylic plate at 5 min intertrial intervals. To record the maximum applied pressure, use the filaments in ascending order, from low to high, until the maximum applied pressure is recorded.¹⁰
   4. When rats exhibit a paw withdrawal response to the stimulation, record the filament number. Determine the withdrawal response in this trial according to the lowest stimulus.
   5. Repeat the same procedure immediately, for a total of three times in succession on the same rat. Convert the filament number into the corresponding force (in grams) and average the values.
3. Plantar Test
   1. Place the rat in a transparent Plexiglas box (divided into four frames, 80 cm × 30 cm × 15 cm) for 30 min for habitation.
   2. Use an infrared beam to stimulate the center of the hindpaw through a glass plate. Adjust the infrared light intensity to obtain an average paw withdrawal response latency of approximately 10 sec. Conduct a trial by depressing a key that turns on the infrared light source and starts a digital solid-state timer. Manipulate the duration of the infrared light beam.
   3. Record the duration of the infrared light when the rats exhibit a paw withdrawal response. The longest duration should not exceed 20 sec in each trial to avoid tissue damage. Use an intertrial interval of at least 5 min to avoid successive stimulation.
   4. Repeat the test with three trials for the left and right hindpaws, and calculate the average for each hindpaw for each rat.
4. Collagenase Lesion Surgery
   1. Anesthetize the rat with 4% isoflurane until loss of the toe-pinch response and somatic responses to surgical stimuli occur. Maintain anesthesia with 1.5 - 2% isoflurane for the duration of surgery.
   2. Place the rat in a stereotaxic device with a simple heating pad to maintain body temperature at 36.5 - 37.5 °C. Apply eye cream on the eyes to prevent dryness while under anesthesia.
   3. Shave the fur with sterilized electric clippers, and make a smooth incision (approximately 2-2.5 cm) with a scalpel along the midline of the scalp. Clean the skin and skull with alternating providence iodine and 75% alcohol solution for disinfection. During the surgical phase, use 75% alcohol to sterilize all devices, tools, and the workbench to maintain sterile conditions. Before that, all surgical materials must be sterilized in a steam autoclave.
   4. Use the sterile gloves and instruments, and drill a small hole (3 mm diameter) in the skull with an electric drill over the VB (including ventral posteromedial thalamic nucleus [VPM] and ventral posterolateral thalamic nucleus [VPL]) of the thalamus (3.0-3.5 mm posterior, 3.0-3.5 mm lateral to bregma, and 5.5-5.8 mm depth from skull surface).
   5. Microinject 0.5 μl of normal saline or 0.125 U of type 4 collagenase solution in the control and experimental groups, respectively.
   6. Keep the injection needle in place for an additional 5 min to allow for drug diffusion.
   7. Use dental cement to fill the hole in the skull, and suture the incision. After suture the incision, apply the local analgesic anesthetics (lidocaine ointment) to the wound, and return them to their home cages.
   8. After surgery, singly house the rats in plastic cages until they maintain sternal recumbency, and keeps warm until recovered from anesthesia.
5. Behavioral Tests after Surgical Recovery
   1. After 7 days of recovery from surgery, repeat the procedures in sections 2.2 and 2.3 for the test phase. Perform the behavioral tests over 4 weeks while monitoring the health and developmental status of the animals.
   2. Monitor the animals' health conditions (e.g., body weight, feeding amount, and free movement) between the control and experimental groups for the post-surgery phase.
6. Perform Cannula Implantation with PE-50 Tubing
   1. Anesthetize the rat with 4% isoflurane, and maintain body temperature at 36.5 - 37.5 °C with a simple heating pad.
   2. With a scalpel, cut two holes (2 cm diameter each) in the midline of the dorsal part of the forelimbs and intersection of the ventral part of the left shoulder and thoracic cavity, respectively.
   3. Dissociate the skin and muscle with a pair of scissors between the two holes.
   4. Connect one end of PE- 50 tubing (20 cm length) to the external jugular vein through the ventral hole. Connect the terminal end of the same PE- 50 tubing to the dorsal hole, and affix to the skin.
   5. Use a syringe to inject saline into the jugular vein to verify that the PE- 50 tubing is not obstructed.
   6. Suture the incision, and inject the rats with 6 mg/kg gentamycin (intraperitoneally).
   7. Flush the tubing every other day after surgery with 0.3 ml of 0.9% saline, followed by 0.1 ml of saline with 20 U/ml heparin.
7. Final Behavioral Test
   1. One week after step 2.6, repeat steps 2.2-2.3 to confirm that behavior is stable compared with step 2.5 after surgical recovery.
8. Radiotracer Injection
   1. Place the rat in a resting cage for 5 - 10 min for adaptation.
   2. Using a splitter, connect PE- 50 tubing to two 1 ml syringes. Fill one syringe with normal saline and fill the other with [¹⁴C]-IAP solution (125 µCi/kg in a volume of 0.3 - 0.5 ml).
   3. Inject the radiotracer into the external jugular vein, and replace the syringe with another syringe filled with 3 M potassium chloride.
   4. Ten seconds after the radiotracer injection, inject 3 M potassium chloride under an overdose of isoflurane, and sacrifice the animals according to standard euthanasia methods (i.e., isoflurane from a vaporizer for 50 min) based on the guidelines of the Academia Sinica Institutional Animal Care and Utilization Committee in Taiwan.
   5. After 1 min, expose the skull, and trim off the remaining muscle. Using rongeurs, peel away the dorsal surface of the skull from the brain. Trim away the sides of the skull using rongeurs. Next, using a spatula, cut the olfactory bulbs and nerve connections along the ventral surface of the brain, and remove the brain.
   6. Use optimal cutting temperature (OCT) compound to freeze the brain in dry ice and methylbutane (approximately -55 °C). Store the brain tissue in a freezer.^{11, 12}
9. Brain Slicing
   1. Orient the tissue in a microtome, with the hindbrain facing down. Use a cryostat to slice the brain into 20 µm-thick sections.
   2. Place the brain slices on microscope slides in a cryostat at -20 °C, with a 240 µm interval between each slice.
   3. Place the microscope slides and five standard filter papers with graded radioactivity into exposure cassettes for 3 days at -20 °C. According to the sequence of the brain slices, arrange the microscope slides from top to bottom. Finally, place the filter papers in the bottom of the cassettes.¹²
   4. Remove the phosphor screen from the exposure cassettes, and use a variable-mode imager to read the phosphor screen and generate images to show [¹⁴C]-IAP uptake for the brain slices.

3. Data Analysis

1. After step 2.9.4, adjust the images using Statistical Parametric Mapping (SPM) and ImageJ software. Reconstruct all of the images using serial coronal sections. Smooth and normalize the images according to a reference rat brain model.^{12, 13}
2. For quantitative assessments, measure the region-of-interest (ROI) of the brain images using ImageJ software to determine the pixel signal intensity, and use statistical software for the analysis.^{12, 13}
3. To investigate the connections between different brain nuclei, use MATLAB correlation analysis software to display radioactivity ratio in an interregional correlation matrix, and visualize the matrices as color maps. Finally, use Pajek software for network analysis.^{12, 13}
4. Use 2 × 5 two-way mixed analysis of variance (ANOVA), with group and weeks as factors, to compare the duration of heat tolerance in the plantar test and mechanical force in the von Frey test in the sham and CPSP groups at baseline and weeks 1 - 5. Use a 2 × 31 two-way ANOVA to measure the radioactivity ratio according to group and brain area. When appropriate, conduct Tukey's Honestly Significant Difference (HSD) post hoc tests. Calculate Pearson correlation coefficients to assess correlations among all of the selected brain areas in the sham and CPSP groups.

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Results

Figure 1A depicts the experimental timeline. Rats were assigned to the sham and CPSP groups for the behavioral tests (i.e., von Frey test and plantar test). The first day of the experiment served as baseline, and tests were repeated at weeks 1 - 5. PE-50 catheterization was performed in the external jugular vein at week 4. Heparin (20 U/ml, 0.1 ml/day) was injected during weeks 4 and 5. Five minutes after the heparin injection, [¹⁴C]-IAP was injected, ...

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Discussion

In the behavioral tests, the CPSP group exhibited reductions of the paw withdrawal threshold in the thermal pain test and mechanical force in the von Frey test at baseline and weeks 1 - 5. The findings were consistent with a previous study.¹⁴

The [¹⁴C]-IAP method relies on the pixel intensity of brain images for the quantitative analysis of different brain slices. To evaluate the data in the brain images, the pixel signal intensity was defined. In the present study, the e...

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Materials

Name	Company	Catalog Number	Comments
Anesthetic:
Isoflurane	Halocarbon Products Corporation	NDC 12164-002-25	4%
Surgery
homeothermic blanket system	Harvard Apparatus	Model 50–7079	body temperature were maintained at 36.5 - 37.5 °C.
10 µl micro syringe	Hamilton	80008, Model 1701SN	injected with collagenase
polyethylene-50 tubing	Becton, Dickinson and Company	427411	catheterized into external jugular vein
1 c.c syringe	Terumo Medical Products	SS-01T	injected with 14C-IAP and saline.
saline (Sodium Chloride 0.9 gm)	Taiwan Biotech Co., LTD.	100-130-0201	To flush the tube
Drugs
type 4 collagenase	Sigma	C5138-500MG	0.125 U
Gentamicin	Sigma	G1264-250MG	6 mg/kg
Heparin	Sigma	H9399	20 U/ml; 0.1 ml/day
14C-iodoantipyrine (IAP)	PerkinElmer	NEC712	125 mCi/kg in 300 ml of 0.9% saline
Potassium chloride	Merck	1.04936.1000	3 M
Behavior system:
von Frey esthesiometer	Fabrication Enterprises, Inc.	Baseline Tactile Monofilaments 12-1666	mechanical hyperalgesia was assessed by measuring the withdrawal response to a mechanical stimulus
plantar test apparatus	IITC Life Science	IITC 390G Plantar Test	Thermal hyperalgesia was assessed by measuring the hind paw withdrawal latency in response to radiant heat.
Brain slice:
Optimal Cutting Temperature compound	Sakura Fintek Inc	4583	embedded the brain
dry ice			frozen in dry ice/methylbutane (approximately −55 °C)
methylbutane	Sigma	M32631-1L	frozen in dry ice/methylbutane (approximately −55 °C)
Cryostat	Leica Biosystems Nussloch GmbH, Germany	Leica CM1850	Coronal brain slice were sectioned on this machine.
Data analyze
exposure cassettes with a phosphor screen	Amersham Biosciences	20 cm x 25 cm	The slices were dried on glass slides and placed alongside five standard filter papers with graded radioactivity. All of the slides were exposed to the cassettes at −20 °C.
γ-counter	Beckman Coulter	Beckman LS 6500 Liquid Scintillation Counter	To measure the radioactivity count of the filter papers.
Typhoon 9410 Variable Mode Imager	GMI, Inc.	WS-S9410	To read  phosphor screen which was exposed by brain slice
Statistical Parametric Mapping (SPM)	Wellcome Centre for Neuroimaging	version 8	all of the brains were averaged to create the final brain template. To determine significant differences between the images in these two groups, the images were derived by subtracting the sham group from the CPSP group.
ImageJ	http://imagej.nih.gov/ij	version 1.46	Adjacent sections were aligned both manually and using Stack- Reg, an automated pixel-based registration algorithm in ImageJ software. All of the original three-dimensionally reconstructed brains were smoothed and normalized to the reference rat brain model.
Matlab	MathWorks	version 2009b	used Pearson correlation coefficients to examine the relationships between the CPSP and sham groups. An inter-regional correlation matrix was calculated across animals from each group.
Pajek	http://Pajek.imfm.si/	version 3.06	Graphical theoretical analysis was performed on networks defined by the above correlation matrices using Pajek software.