The authors would like to acknowledge the contributions of the University of Kentucky Center for Microelectrode Technology (CenMeT), and the Ohio State University Laboratory Animal Resource Center (ULAR).

Piglets (Sus scrofa) are received through a local farm pre-approved by The Ohio State University (OSU) Institutional Animal Care and Use Committee (IACUC). Following approval of the protocol, animal experimentations are done in accordance with IACUC policy.
1. Piglets and Piglet Handling
<ol>
	<li>Utilize male and female piglets in a systematic and randomized manner to eliminate any potential sex-based confounders in accordance with ARRIVE guidelines19. 
	NOTE: Since the period of maximal brain growth is within 3-5 days of piglet birth, experimentation is done solely with piglets 3-5 days old.</li>
	<li>Ensure piglets arrive in the vivarium at least 24 h before experimentation to allow acclimation to the environment. 
	NOTE: Trained veterinary staff provides routine animal care. The piglets are kept in individually temperature-maintained, continuously monitored cages and receive a nutritionally-complete milk replacer ad libitum to prevent hypoglycemia. The piglets are also kept without milk replacement (nil per os), for at least 3 h prior to anesthesia and are supplied with blankets and toys to ensure normal levels of stimulation. If possible, keep multiple piglets in the same cage to allow socialization.</li>
</ol>
2. Development and Customization of MEAs for AIN Studies in a Piglet Model
NOTE: This technology uses enzyme-based MEAs that are pre-coated with enzyme and electroplated with m-phenylenediamine dihydrochloride (mPD). The electrodes were custom designed with a 40-mm rigid shaft and manufactured for use in piglets (Figure 1).
<ol>
	<li>To avoid redundancy, please see the detailed description of MEA preparation and calibration as previously described15 (Figure 2).</li>
</ol>
3. Anesthesia and Use of Custom Stereotaxic Apparatus for the Piglet
<ol>
	<li>Anesthetize animals using an anesthesia workstation with an appropriate ventilator and monitoring devices, and monitor physiologic parameters such as pulse oximetry, non-invasive blood pressure, electrocardiography, and temperature throughout the entirety of the experiment as previously described19. Intubate and ventilate the piglets and administer sevoflurane anesthesia at 1 minimum alveolar concentration (MAC) (approximately 2.5-3%) for 3.5 h. Ensure that trained laboratory staff members are present for these experiments.&#160;Fur overlying the surgical area is removed using electric clippers prior to preparation of the skin. 
	NOTE: The concentration and duration of anesthetic used allows the experiment to simulate the time-length of actual anesthesia exposure during a surgical procedure. Additionally, sevoflurane is the most commonly utilized general anesthetic in the pediatric population making the investigation surrounding its safety of utmost importance.</li>
	<li>Before placement into the stereotaxic frame, start a rocuronium loading dose of 2.5 mg/kg and an infusion of 1.5 mg/kg/h to prevent animal movement while secured in the frame.
	<ol>
		<li>Place the piglet in the piglet-specific stereotaxic frame once an adequate depth of anesthesia is confirmed by toe-pinch.</li>
		<li>Provide adequate padding within the stereotaxic frame by placing the piglet on a forced- air warming pad with additional padding (e.g., fluidized positioner) to prevent pressure ulcers.</li>
		<li>Place the teeth of the upper mandible over the tooth bar (Figure 3). 
		NOTE: The tooth bar should be at a sufficient level to hold the skull very firmly in place.</li>
		<li>Fix and tighten the penetrating ear bars within the ears, taking care to ensure that the piglet is in the midline position. Position the pointed tips of the lateral holds within the ear canal and insert the ear bars firmly enough to hear the &#34;pop&#34; sound associated with the penetration of the tympanic membrane. Firmly attach the ear bars to the skull and insert to equal depth on each side in order to prevent movement of the skull during the experiment (Figure 4, Panel A). 
		NOTE: It is vitally important to keep the piglet warm (~ 37.8-38.6 &#176;C) and continuously monitor the temperature during the entire procedure for maintenance of normothermia. This can be accomplished via a blanket and/or a heat lamp. Be sure to place the heat lamp at an appropriate distance to avoid burning of the animal&#39;s skin.</li>
	</ol>
	</li>
	<li>Create a 4-6 cm midline incision along the skull using caution to avoid scoring the skull with the scalpel. Once the incision is made, use gentle retraction and blunt dissection to elevate the scalp from the skull. Gently scrub the skull with a gauze pad to remove any connective tissue and expose the suture lines (Figure 4, Panel B). 
	NOTE: It is not necessary to maintain sterility during non-survival experiments. However, sterility must be maintained during survival experiments.</li>
	<li>Further reflect the scalp, if necessary, to expose the area of interest and determine the intended location for the craniotomy (Figure 5, Panel A). Use a surgical drill to create a craniotomy window of approximately 0.25 cm2 (may be larger or smaller depending on experimental goals) overlying the structure of interest, using caution not to injure the dura or the underlying brain (Figure 5, Panel B). Use fine surgical scissors to excise the dura overlying the brain tissue (Figure 5, Panel C).</li>
	<li>Position the electrode as vertically as possible over the bregma by securing the metal arm of the headstage to the micromanipulator of the piglet stereotax. Lower the electrode as much as possible without touching the surface of the skull. Record the coordinates of the bregma (Figure 6, Panel A).
	<ol>
		<li>Determine the anterior-posterior and medial-lateral coordinates as well as the depth of the structure of interest as they relate to the bregma. Determine the stereotaxic coordinates using a species and age-appropriate stereotaxic atlas. In this case, use a stereotaxic atlas developed specifically for piglets20.</li>
		<li>Reposition the electrode so that it has the proper anterior-posterior and medial-lateral location, ensuring that both the microelectrode and the apparatus are perpendicular to the surface. Place the pseudo-reference electrode under the scalp, ensuring contact with the animal (Figure 6, Panel B).</li>
		<li>Slowly and gently, lower the electrode to the appropriate depth into the brain using the stereotaxic arm. For the final 2 mm, use a hydraulic microdrive to further drive the electrode to the exact location (Figure 6, Panel C). 
		NOTE: The electrode position should overlie the craniotomy window. The electrode depth will vary depending on the brain structure of interest. It is not necessary to close the incision upon completion of data collection in non-survival experiments.</li>
	</ol>
	</li>
</ol>
4. Measurement of Extracellular Glutamate Under Sevoflurane Anesthesia
<ol>
	<li>Ensure the piglet is under continuous physiologic monitoring throughout the entirety of this procedure.&#160;Piglets are anesthetized inhalationally (via face cone) in preparation for the procedure.&#160;</li>
	<li>After implantation of the MEA, wait 30 min to allow the electrode to reach baseline to ensure that correct measurement will be obtained for 3 h (Figure 7).</li>
	<li>0.25% bupivacaine (1 mL/kg) is administered subcutaneously at the site of the surgery for postoperative pain management. In addition, sustained-release buprenorphine is given subcutaneously q72h as needed.</li>
</ol>
5. Perfusion and Sacrifice
<ol>
	<li>Perform the perfusion and brain tissue collection procedures as previously described21.&#160;For non-survival surgeries, animals are euthanized immediately after experimentation while still under general anesthesia.</li>
	<li>Take gross cross-sections of the fixed piglet brain and use light microscopy to visualize the track of the electrode as previously described22 to allow verification of MEA placement, ensuring proper placement in the area of interest.</li>
</ol>

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Greg Gerhardt is the principal owner of Quanteon LLC. Jorge Quintero and Jason Burmeister have served as consultants to Quanteon LLC.

From the start of the experiment, the piglet&#39;s physiological homeostasis must be maintained as described in this lab&#39;s prior publication21. Minimal monitoring should include pulse oximetry, electrocardiography, capnography, non-invasive blood pressure, and temperature. Trained investigators are required so that physiologic perturbations (e.g., hypo/hyperthermia, hypoxia, hypotension, arrhythmia) can be appropriately corrected.
Prior to induction, in vitro MEA calibrations are performed to establish functionality and selectivity of the MEA under known conditions. The calibration and plating of MEAs is critical for effective use of the technology. There are many potential errors that can arise during calibration. Calibration can identify these issues as well as improper plating, which leads to incorrect interferent response. A more detailed tabular account of errors that may occur in MEA response has been compiled, along with notable causes and suggested solutions, which should prove a useful instrument for likely troubleshooting (Table 1). It is important to note that prior to both calibration and plating, the glass reference electrode should be checked for the presence of air bubbles or white discoloration, as either will negatively impact MEA function and recording accuracy.
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Symptom</td>
			<td>Cause</td>
			<td>Corrective Action</td>
		</tr>
		<tr>
			<td rowspan="2">No Signal</td>
			<td>Electrode not connected</td>
			<td>Properly connect electrode to headstage and headstage to FAST amperometry system.</td>
		</tr>
		<tr>
			<td>No power to the FAST amperometry system</td>
			<td>Turn on power switch on back of FAST system</td>
		</tr>
		<tr>
			<td rowspan="5">Signal Noise</td>
			<td rowspan="2">Electrode contaminated by blood</td>
			<td>Continuously irrigate the brain surface during electrode insertion</td>
		</tr>
		<tr>
			<td>Rinse the electrode immediately in dH2O</td>
		</tr>
		<tr>
			<td>Enzyme coating is loose</td>
			<td>Clean and recoat the electrode</td>
		</tr>
		<tr>
			<td>Reference electrode was not inserted or coated</td>
			<td>Coat and place the reference electrode farther under the scalp</td>
		</tr>
		<tr>
			<td>Electrode is detecting movement of brain surface</td>
			<td>Usually occurs in superficial structures. Insert the electrode deeper (1 mm at a time) if possible</td>
		</tr>
		<tr>
			<td rowspan="2">Animal Movement</td>
			<td>Animal is inadequately secured</td>
			<td>Move the animal in the posterior direction to better secure earbars on the skull. If necessary, elevate the torso to allow for better body alignment.</td>
		</tr>
		<tr>
			<td>Animal is inadequately anesthetized</td>
			<td>Verify the integrity of the anesthetic equipment. Titrate the anesthetic to an effective dose and administer an intramuscular rocuronium dose (5 mg/kg)</td>
		</tr>
		<tr>
			<td rowspan="3">Inaccurate electrode placement</td>
			<td>Electrode is not correctly aligned</td>
			<td>Readjust the electrode while maintaining proper connection to the headstage.</td>
		</tr>
		<tr>
			<td rowspan="2">Stereotaxic coordinates are inaccurate</td>
			<td>Ensure that the piglet atlas being referenced does not use another reference point or plane of alignment.</td>
		</tr>
		<tr>
			<td>Be careful not to obscure the suture marks by scoring the skull.</td>
		</tr>
	</tbody>
</table>
Table 1: Instructions for troubleshooting MEA use in piglets. Possible causes and corrective actions to assist with optimization and troubleshooting.
A stereotaxic atlas for the piglet is used to determine the stereotaxic coordinates of the area of interest with respect to a known point such as bregma18. Ear bars should be properly secured to ensure that the skull is level and fully immobilized. Care should be taken during the midline incision of the scalp to avoid scoring the skull as this may affect visualization of the suture lines. The craniotomy window should be large enough to accommodate the MEA.
This protocol presents a number of technical challenges that require a well-stocked operating suite and an investigator/team skilled in the surgical and anesthetic aspects of the protocol. The model additionally presents financial limitations in that the piglet model is more expensive than the rodent model; however, it is significantly less costly than the use of non-human primates, which can cost thousands of dollars. The use of MEA technology presents its own challenges, as the procedure of coating and plating the electrodes manually require a skilled investigator or assistant to ensure sufficient selectivity and reliable function. The microelectrodes themselves are fragile, as they are made of ceramic, and thus easily damaged if proper caution is not observed. Microelectrodes are subject to interference from other electrical devices, which can create noise in recordings, and from blood at the operative site, which can occlude the recording sites. The need for specialized equipment presents an additional burden as a stereotaxic surgical frame must be custom built to immobilize the piglet skull during implantation. The stereotaxic frame, glutamate oxidase, and the electrodes themselves are all costly. Additionally, the lack of a piglet stereotaxic atlas from within the last decade poses technical limitations that require particular expertise to determine the specific location of deep structures in the piglet brain. Development of a new stereotaxic atlas, perhaps using magnetic resonance imaging, would greatly enhance the ability to use this technology in piglets.
The piglet is a clinically relevant model for the study of AIN largely due to the parallels that exist between this species and the human neonate, as both possess similar brain structure and development. Unlike more commonly used models such as mice or rats, the piglet has a greater CNS similarity to humans, which lends to the translatability of the model&#39;s results. The piglet model is additionally cheaper and involves less complicated handling than a non-human primate model. The piglet model is intended to examine the process by which anesthesia might induce developmental neurotoxicity, measure its contribution to neurological damage, and combat the issue of damage caused by confounding variables. For instance, hypoxia may be misconstrued for damage caused by anesthetics as it has global effects on the brain. The piglet is utilized with the same surgical and anesthetic conditions as those used in human medicine to ensure fidelity of results.
The use of ceramic-based MEA technology eliminates several of the disadvantages associated with the contemporary technique of microdialysis. Microdialysis has limited temporal and spatial resolution in comparison to amperometric methods such as the MEA, which can continuously record glutamate events in multiple, microscopic regions at up to 10 Hz23. This rapid sampling rate eliminates the confounding factor of localized neurotransmitter diffusion that is inherent to slow-sampling methods like microdialysis24. Additionally, the MEA is a less invasive method than a microdialysis probe, which can cause significant gliosis during insertion and may alter neurotransmitter activity at the insertion site22.
Previous studies utilizing a range of mammalian models, measurement techniques, and regions of the brain, have demonstrated basal glutamate levels comparable to those found using this technique. This suggests that MEA technology, when adapted to the piglet model, provides valid recordings of in vivo glutamate concentration (Table 2).
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Author (Year)</td>
			<td>Recording Technique</td>
			<td>Animal Model</td>
			<td>Age</td>
			<td>Brain Region(s)</td>
			<td>Mean Basal Glutamate Concentration (&#181;M)</td>
		</tr>
		<tr>
			<td>Hascup et al. (2008)23</td>
			<td>MEA (Enzyme-based)</td>
			<td>Rodent</td>
			<td>20 - 24 weeks&#160;</td>
			<td>Prefrontal Cortex, Striatum&#160;</td>
			<td>3.3 &#177; 1.0; 5.0 &#177; 1.2</td>
		</tr>
		<tr>
			<td>Hascup et al. (2010)25</td>
			<td>MEA (Enzyme-based)</td>
			<td>Rodent</td>
			<td>3 - 6 months</td>
			<td>Hippocampus&#160;</td>
			<td>4.7 - 10.4</td>
		</tr>
		<tr>
			<td>Rutherford et al. (2007)9</td>
			<td>MEA (Enzyme-based)</td>
			<td>Rodent</td>
			<td>&#160;3 - 6&#160;months&#160;</td>
			<td>Prefrontal Cortex, Striatum</td>
			<td>44.9&#160;&#177;&#160;4.7; 7.3&#160;&#177;&#160;0.9&#160;</td>
		</tr>
		<tr>
			<td>Miele et al. (1996)26</td>
			<td>Microdialysis (Enzyme-based)</td>
			<td>Rodent</td>
			<td>-</td>
			<td>Striatum&#160;</td>
			<td>3.6&#160; &#177; 0.5</td>
		</tr>
		<tr>
			<td>Day et al. (2006)27</td>
			<td>MEA (Enzyme-based)</td>
			<td>Rodent</td>
			<td>3 - 6 months</td>
			<td>Frontal Cortex, Striatum&#160;</td>
			<td>1.6 &#177; 0.3 ;1.4&#160;&#177;&#160;0.2&#160;</td>
		</tr>
		<tr>
			<td>Quintero et al. (2007)28</td>
			<td>MEA (Enzyme-based)</td>
			<td>Non-Human Primate</td>
			<td>5.3 - 5.5 years&#160;</td>
			<td>Premotor Cortex, Motor Cortex</td>
			<td>3.8 &#177; 1.7; 3.7 &#177; 0.9&#160;</td>
		</tr>
		<tr>
			<td>Stephens et al.&#160; (2010)29</td>
			<td>MEA [Spencer-Gerhardt-2 (SG-2)]&#160;</td>
			<td>Non-Human Primate</td>
			<td>&#160;11 - 21 years&#160;</td>
			<td>Putamen</td>
			<td>8.53</td>
		</tr>
		<tr>
			<td>Kodama et al. (2002)30</td>
			<td>Microdialysis (Enzyme-based)</td>
			<td>Non-Human Primate</td>
			<td>-</td>
			<td>Prefrontal Cortex&#160;</td>
			<td>1.29 - 2.21</td>
		</tr>
		<tr>
			<td>Galvan et al. (2003)31</td>
			<td>Microdialysis (Enzyme-based)</td>
			<td>Non-Human Primate</td>
			<td>Juvenile&#160;</td>
			<td>Striatum</td>
			<td>28.74 &#177; 2.73</td>
		</tr>
		<tr>
			<td>During and Spencer (1993)32</td>
			<td>Microdialysis (Enzyme-based)</td>
			<td>Human</td>
			<td>18 - 35 years&#160;</td>
			<td>Hippocampus&#160;</td>
			<td>20.3 &#177; 6.6</td>
		</tr>
		<tr>
			<td>Reinstrup et al. (2000)33</td>
			<td>Microdialysis (Enzyme-based)</td>
			<td>Human</td>
			<td>-</td>
			<td>Frontal Cortex</td>
			<td>16 &#177; 16</td>
		</tr>
		<tr>
			<td>Cavus et al. (2005)34</td>
			<td>Microdialysis (Enzyme-based)</td>
			<td>Human</td>
			<td>15 - 52 years</td>
			<td>Neocortex</td>
			<td>2.6 &#177; 0.3</td>
		</tr>
	</tbody>
</table>
Table 2. Comparison of basal extracellular glutamate levelsacross various animal models. A selected review of studies establishing normal extracellular glutamate levels in healthy awake and anesthetized animals using microdialysis or microelectrodes.
The use of MEA technology to monitor in vivo glutamate concentrations in the piglet model can allow for the future evaluation of piglet neurological outcomes post-anesthesia. Survival experiments have been planned, which will further an understanding of the long-term impact of anesthesia on the neurocognitive well-being of human neonates. Survival experiments will allow for behavioral testing and monitoring of glutamate changes long after anesthesia exposure. It is also common for children to undergo anesthesia in conditions where they might experience physiological stress in the form of surgical intervention. Future studies addressing the influence of surgery in terms of neurological injury and increase in neurotoxicity would allow for more accurate modeling of a common clinical setting for children. The use of alternate animal models is also feasible, as is the study of these various models through chronic implantation, allowing us to track behavioral changes associated with neurotoxicity. MEA technology itself is versatile, so future study need not be limited to analysis of glutamate levels (e.g., GABA, choline, lysine, etc. could be analyzed).

Every year, millions of children undergo anesthesia for both invasive and non-invasive procedures in the United States1. For years, anesthesia providers have reassured parents of the safety of anesthetics, even in small children and neonates. However, in 1999 it was found that transient blockage of the N-methyl-D-aspartate (NMDA) subtype of glutamate receptors during early life could cause widespread neuronal apoptosis in rats2. Recently, the FDA released a drug safety communication that will require the labels of anesthetic drugs to include a warning about general anesthetics and their potential negative effect on the developing brains of children younger than 3 years old (U.S. Food and Drug Administration, 2017). However, there is still a need to elucidate possible mechanisms and potential neuroprotective measures.
Normal activity of neurotransmitters such as glutamate and gamma-amino butyric acid (GABA) are critical for normal neurodevelopment to occur. Although most of the pathways involved in AIN are still elusive, neurotransmitter systems are very likely to be involved since anesthetics are known to modulate these pathways to produce unconsciousness. In particular, the excitatory neurotransmitter glutamate causes excitotoxicity when its activity is dysregulated. This neurotransmitter is normally involved in neurogenesis, neural plasticity, synaptic and neural growth, and a number of other critically important brain functions. However, prolonged activation of glutamate receptors can cause excitotoxicity and neuronal apoptosis, particularly under stress conditions such as surgery, oxygen deprivation, and reduced energy availability3. Binding of glutamate to the NMDA receptor has been shown to cause Na+ and Cl&#8722; influx. The subsequent depolarization is thought to lead to Ca2+ channel opening and release of intracellular Ca2+ stores4. This dysfunction likely leads to a cascade of metabolic derangements which eventually decrease neuronal proliferation, increase inflammation, and lead to neuronal death. Despite these hypotheses, the true mechanism(s) of AIN remain unclear5. Because of its role in apoptosis, glutamate dysregulation represents a novel pathway that may contribute to the mechanism of previously documented neuronal apoptosis, a feature of AIN.
One of the hindrances on the study of neuronal processes is their high complexity, especially in the setting of neuronal development. The first few months of life are the period of maximal vulnerability to injury, during which most of the important steps of neuronal development such as physiologic apoptosis (neuronal pruning), synaptogenesis, gliogenesis, and myelination take place6. Given the complex nature of neuronal communication and the difficulty of studying these processes without disrupting normal CNS function, new technologies have been developed which aim at the in vivo detection and quantification of important elements of neuronal communication.
Enzyme-linked MEA technology was used in this study as a novel way to study the mechanisms of AIN in a clinically-relevant piglet model. This technology can be used to study complex in vivo electrochemical brain processes, including glutamate dysregulation. The incorporated 4-channel platinum recording sites of the MEAs (2 glutamate-sensitive sites and 2 sentinel sites) allow self-referencing, which contributes to detection accuracy. In addition, an exclusion layer is applied to each electrode, conferring selectivity by preventing other interfering molecules from being detected7. Moreover, the low-profile design of the MEA allows for minimal tissue trauma compared to earlier technologies. This same feature confers to MEAs a higher spatial resolution, which facilitates the study of microscopic regions in the brain. For example, discrete regions of the hippocampus (dentate gyrus, CA1, CA2) can be specifically studied8. Specific details on the functionality of MEAs have been previously described9.
In comparison to MEA electrochemistry, microdialysis incorporates a membrane placed between the solution of interest and a solution of similar composition, allowing detection of extracellular fluid changes10. Although microdialysis is a mainstay of neurochemistry and has long been used for the detection of neurotransmitters, it has the disadvantage of low time resolution, delayed detection of glutamate change, and significant tissue trauma11.
MEAs can indirectly detect neurotransmitters such as glutamate, acetylcholine, and choline, by using appropriate oxidase enzymes that produce electroactive reporter molecules such as H2O2 or O212,13.
MEA technology has been widely used in rats and non-human primates for the study of neurotoxicity in the context of pathophysiological processes other than AIN7,14. Among some of these pathophysiological processes, MEA technology has been used for the study of Alzheimer&#39;s disease, epilepsy, traumatic brain injury, and the effect of pharmacological compounds on synaptic communication8,15,16,17. Although MEAs have been used to study these pathologies in rats and non-human primates, the high developmental similarity between humans and piglet brains makes the adaptation of the MEA technology in piglets a highly suitable technique for the study of AIN mechanism(s)18.

<table><tbody><tr><td>Advance Liqui-Wean Pig Milk Replacer</td><td>PBS Animal Health</td><td>292-13</td><td></td></tr><tr><td>Piglet Anesthesia Face-Cone Mask</td><td>VetEquip</td><td>921428</td><td></td></tr><tr><td>Integra SL Anesthesia Workstation</td><td>DRE Veterinary</td><td>2350</td><td>This anesthesia workstation is chosen to best mimic the clinical monitoring experienced by pediatric patients in the operating room. Any anesthesia machine can be used as long as it allows for sufficient physiologic monitoring and intervention.</td></tr><tr><td>Sevoflurane</td><td>Ultane</td><td>0074-4456-04</td><td></td></tr><tr><td>Rocuronium Bromide Injection</td><td>Hospira</td><td>0409-9558-05</td><td></td></tr><tr><td>Medfusion 4000 IV Infusion&amp;nbsp;</td><td>Smiths Medical</td><td></td><td></td></tr><tr><td>Model 1530 Heavy-Duty Research Model Stereotax</td><td>Kopf</td><td></td><td>custom made</td></tr><tr><td>Model 1541 Piglet Adaptor</td><td>Kopf</td><td></td><td>custom made</td></tr><tr><td>Infrared Spot Lamp</td><td>Amazon</td><td>B000HHQ94C</td><td></td></tr><tr><td>Bair Hugger Torso Blanket</td><td>3M</td><td>540</td><td></td></tr><tr><td>Bair Hugger</td><td>3M</td><td>750</td><td></td></tr><tr><td>Sterile Alcohol Prep Pad</td><td>Fisherbrand</td><td>22-363-750</td><td></td></tr><tr><td>Carbon Steel Rib-Back Surgical Blade</td><td>Bard-Parker</td><td>#10</td><td></td></tr><tr><td>Scalpel Handel</td><td>Havel&#039;s</td><td>HAN-G4</td><td></td></tr><tr><td>Surgical Scissors</td><td>World Precision Instruments</td><td>504615</td><td></td></tr><tr><td>Mosquito Forceps</td><td>Sklar Surgical Instruments</td><td>17-1225</td><td></td></tr><tr><td>Gauze Pads</td><td>Fisherbrand</td><td>22-246-069</td><td></td></tr><tr><td>Adson Tissue Forceps</td><td>Teleflex</td><td>181223</td><td></td></tr><tr><td>Dremel 111 Engraving Cutter</td><td>Amazon</td><td>Dremel 111</td><td></td></tr><tr><td>Microelectrode Array</td><td>Center for Microelectrdoe Technology, University of Kentucky</td><td></td><td>S2 4Ch MEA; custom made</td></tr><tr><td>Headstage</td><td>Quanteon</td><td></td><td>2pA/mV</td></tr><tr><td>Wire, silver, PFA, .008&quot; Bare, .0110&quot; coated</td><td>A-M Systems</td><td>786500</td><td></td></tr><tr><td>Fine Micromanipulator</td><td>Narishige Scientific Instrument Lab</td><td>MO-8</td><td></td></tr></tbody></table>

adaptation of microelectrode array technology for the study of anesthesia-induced neurotoxicity in the intact piglet brain

Every year, millions of children undergo anesthesia for a multitude of procedures. However, studies in both animals and humans have called into question the safety of anesthesia in children, implicating anesthetics as potentially toxic to the brain in development. To date, no studies have successfully elucidated the mechanism(s) by which anesthesia may be neurotoxic. Animal studies allow investigation of such mechanisms, and neonatal piglets represent an excellent model to study these effects due to their striking developmental similarities to the human brain.
This protocol adapts the use of enzyme-based microelectrode array (MEA) technology as a novel way to study the mechanism(s) of anesthesia-induced neurotoxicity (AIN). MEAs enable real-time monitoring of in vivo neurotransmitter activity and offer exceptional temporal and spatial resolution. It is hypothesized that anesthetic neurotoxicity is caused in part by glutamate dysregulation and MEAs offer a method to measure glutamate. The novel implementation of MEA technology in a piglet model presents a unique opportunity for the study of AIN.

This proof-of-concept study with enzyme-based ceramic MEA technology in a piglet model can provide exceptional insight into the glutamate dynamics underlying AIN. This study further demonstrates that enzyme-based MEA technology can be successfully adapted in the piglet model to measure physiologic and anesthesia-associated changes in neurotransmitter activity with high sensitivity, and high spatial and temporal resolution. Physiologic homeostasis was maintained throughout our experiments using clinically relevant methods and standards, and no piglet exhibited signs of physiologic perturbations.
The data obtained indicates the ability of MEAs to precisely and spatially resolve neurotransmitter measurements in cortical and sub-cortical brain structures. The use of a stereotaxic apparatus enables clear identification of a reference surface structure (bregma) in order to consistently locate the region of interest, regardless of individual differences in piglet size and anatomy. Clear visualization of the sutures facilitates consistent regional placement of the MEA with accuracy in the micrometer range (Figure 4). Obtaining access to the cortical surface of the brain is minimally traumatic with negligible bleeding, ensuring that any in vivo glutamate dynamics are not due to unintentional systemic or local insult (Figure 5). The custom, rigid MEA is then aligned perpendicular to the frontal plane of the piglet (Figure 6). Failure to properly align the MEA prior to insertion may prevent accurate spatial recording of the targeted region, especially for subcortical regions.
Real-time in vivo glutamate measurements were taken in the hippocampi of 3-4-day old piglets (n = 4) under 2.5-3% sevoflurane anesthesia (approximately 1 MAC). Amperometry measurements were recorded at 4 Hz and converted to concentration using a linear regression based on calibration parameters (Figure 8, Panel A). For each time point, the signals from the two glutamate-sensitive sites were averaged before subtracting the averaged sentinel signal to yield a corrected glutamate signal. These continuous measurements were smoothed by applying a moving average to better visualize the overall trend over time (Figure 8, Panel B). The mean basal glutamate concentration was calculated to be 4.61 &#177; 0.02 &#181;M and remained relatively stable over the course of anesthetic exposure. Transient glutamatergic activity was identified in one animal by analyzing peaks in the signal that were not correlated with the sentinel signal (R2 &#60; 0.5) and exceeded a signal-to-noise ratio of 3 (Figure 9, Panel A). A total of 116 transient peaks were detected over a period of 3.5 h (Figure 10, Panel A). The amplitude of the resulting transient peaks was generally observed to be within the 1 &#181;M range (Figure 10, Panel B). In order to quantify the duration of each transient, the time (t80) required for each maximum peak value to decay 80% was obtained (Figure 9, Panel B). The mean t80 of all glutamate transients during the 3.5 h recording period was 4.68 &#177; 0.82 s (Figure 10, Panel C). These data demonstrate that it is possible to accurately measure both prolonged and transient neurotransmitter activity in a subcortical region of the anesthetized piglet brain.
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/57391/57391fig1.jpg" /> 
Figure 1: Visual comparison of SG-2 microelectrode array types. SG-2 arrays contain two glutamate-sensitive sites and two glutamate-insensitive sentinel sites (150 &#181;m x 20 &#181;m per site).(A) A flexible-shaft microelectrode array is shown on the left. The rigid-shaft microelectrode array was custom-designed for use in piglets and permits deeper implantation in large animals. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57391/57391fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/57391/57391fig2.jpg" /> 
Figure 2: Overview of microelectrode array preparation and calibration process. The total MEA preparation and calibration last approximately one week. The coating enzyme, exclusion layer, and calibration analytes are specific to the neurotransmitter of interest. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57391/57391fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/57391/57391fig3.jpg" /> 
Figure 3: Placement of piglet in the stereotaxic apparatus. The piglet mouth is placed on mouth bar directly posterior to the canine teeth. The penetrating ear bars are inserted into the ear canals to secure the posterior end of the skull. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57391/57391fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/57391/57391fig4.jpg" /> 
Figure 4: Placement of piglet in the stereotaxic apparatus for craniotomy. (A) The piglet&#39;s head is tightly secured within the custom stereotaxic frame, ensuring consistent placement of the MEA. Equidistant placement of penetrating ear bars is visible. (B) Midline anterior-posterior incision along the scalp. Scoring of the skull was avoided to visualize coronal and sagittal sutures and optimize visualization of bregma. The scale bar is shown to indicate the relative size of the incision and the location of craniotomy window. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57391/57391fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 5" class="xfigimg" src="/files/ftp_upload/57391/57391fig5.jpg" /> 
Figure 5: Craniotomy for access to the hippocampus. (A) The scalp further reflected to expose the approximate location of the MEA insertion according to stereotaxic coordinates. The circled area is marked (black dot) to guide the craniotomy. (B) The craniotomy window (0.25 cm2) with skull flap removed to expose the underlying dura mater. (C) The meninges carefully removed to expose superficial cerebral cortex without tissue trauma. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57391/57391fig5large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 6" class="xfigimg" src="/files/ftp_upload/57391/57391fig6.jpg" /> 
Figure 6: MEA positioning and insertion into the hippocampus. (A) Placement of MEA at the bregma to determine a relative stereotaxic location of the hippocampus. (B) Stereotaxic placement of the MEA at the brain surface to determine the hippocampus insertion depth. Silver pseudo-reference electrode securely placed under scalp (indicated by arrow). (C) the MEA inserted at the appropriate depth to obtain real-time, in vivo extracellular glutamate measurements in the hippocampus. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57391/57391fig6large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 7" class="xfigimg" src="/files/ftp_upload/57391/57391fig7.jpg" /> 
Figure 7: MEA behavior during the 30-min baselining period. The initial rapid increase corresponds to the descent of the MEA into the hippocampus using the micromanipulator. The baseline period begins once the MEA has reached the appropriate depth (dotted line). Extracellular glutamate measurements will decrease over a period of 30 min and should not be interpreted as physiologic readings. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57391/57391fig7large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 8" class="xfigimg" src="/files/ftp_upload/57391/57391fig8.jpg" /> 
Figure 8: Real-time extracellular glutamate measurements in the hippocampus of a neonatal pig under sevoflurane anesthesia. (A) The moving average of the glutamate concentration in the hippocampus of one neonatal pig under sevoflurane anesthesia (using 10 data points). Measurements were taken at 4Hz for 3 h after a brief 30 min baselining period. (B) Smoothing of glutamate measurements using a moving average of 100 points every 15 min to better visualize the trend. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57391/57391fig8large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 9" class="xfigimg" src="/files/ftp_upload/57391/57391fig9.jpg" /> 
Figure 9: Identification of transient glutamate activity in the hippocampus of a neonatal pig under sevoflurane anesthesia. (A) Transient glutamate peaks (in red) are indicated on the real-time glutamate tracing. Peaks were considered significant when the signal to noise ratio exceeded 3 and their signal was not correlated with the sentinel signal (R2 &#60; 0.5). (B) A representative transient peak identified in Figure 9, Panel A. Dotted lines indicate the total duration required for the peak to decay 80%. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57391/57391fig9large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 10" class="xfigimg" src="/files/ftp_upload/57391/57391fig10.jpg" /> 
Figure 10: Characterization of glutamate transients in the hippocampus of a neonatal pig under sevoflurane anesthesia. (A) A number of transient glutamate peaks in 15 min bins. Peaks were considered significant when the signal to noise ratio exceeded 3 and their signal was not correlated with the sentinel signal (R2 &#60; 0.5). (B) The amplitude of transient glutamate peaks. Error bars indicate the standard error of the mean. (C) Mean T80 of transient glutamate peaks. Error bars indicate the standard error of the mean. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/57391/57391fig10large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Adaptation of Microelectrode Array Technology for the Study of Anesthesia-induced Neurotoxicity in the Intact Piglet Brain at JoVE.com

Adaptation of Microelectrode Array Technology for the Study of Anesthesia-induced Neurotoxicity in the Intact Piglet Brain

This study explores the novel use of enzyme-based microelectrode array (MEA) technology to monitor in vivo neurotransmitter activity in piglets. The hypothesis was that glutamate dysregulation contributes to the mechanism of anesthetic neurotoxicity. Here, we present a protocol to adapt MEA technology to study the mechanism of anesthesia-induced neurotoxicity.

Every year, millions of children undergo anesthesia for a multitude of procedures. However, studies in both animals and humans have called into question ...

adaptation-microelectrode-array-technology-for-study-anesthesia

Nanyang Technological University

Research

JoVE Journal

Neuroscience

9.4K Views.  Ohio State University College of Medicine. Deze studie verkent het nieuwe gebruik van enzym gebaseerde micro-elektrode matrix (MEA) technologie om te controleren in vivo neurotransmitter activiteit bij biggen. De hypothese was dat glutamaat disregulatie draagt bij aan het mechanisme van verdoving neurotoxiciteit. Hier presenteren we een protocol aan te passen van MEA technologie om te bestuderen van het mechanisme van anesthesie-geïnduceerde neurotoxiciteit.

Video: Adaptation of Microelectrode Array Technology for the Study of Anesthesia-induced Neurotoxicity in the Intact Piglet Brain

A Piglet Model of Neonatal Hypoxic-Ischemic Encephalopathy

Birth asphyxia, which causes hypoxic-ischemic encephalopathy (HIE), accounts for 0.66 million deaths worldwide each year, about a quarter of the world&#8217;s 2.9 million neonatal deaths. Animal models of HIE have contributed to the understanding of the pathophysiology in HIE, and have highlighted the dynamic process that occur in brain injury due to perinatal asphyxia. Thus, animal studies have suggested a time-window for post-insult treatment strategies. Hypothermia has been tested as a treatment for HIE in pdiglet models and subsequently proven effective in clinical trials. Variations of the model have been applied in the study of adjunctive neuroprotective methods and piglet studies of xenon and melatonin have led to clinical phase I and II trials1,2. The piglet HIE model is further used for neonatal resuscitation- and hemodynamic studies as well as in investigations of cerebral hypoxia on a cellular level. However, it is a technically challenging model and variations in the protocol may result in either too mild or too severe brain injury. In this article, we demonstrate the technical procedures necessary for establishing a stable piglet model of neonatal HIE. First, the newborn piglet (&#60; 24 hr old, median weight 1500 g) is anesthetized, intubated, and monitored in a setup comparable to that found in a neonatal intensive care unit. Global hypoxia-ischemia is induced by lowering the inspiratory oxygen fraction to achieve global hypoxia, ischemia through hypotension and a flat trace amplitude integrated EEG (aEEG) indicative of cerebral hypoxia. Survival is promoted by adjusting oxygenation according to the aEEG response and blood pressure. Brain injury is quantified by histopathology and magnetic resonance imaging after 72 hr.

Hypoxic-ischemic encephalopathy following perinatal asphyxia can be studied using animal models. We demonstrate the procedures necessary for establishing a piglet model of neonatal hypoxic-ischemic encephalopathy.

Birth asphyxia, which causes hypoxic-ischemic encephalopathy (HIE), accounts for 0.66 million deaths worldwide each year, about a quarter of the ...

Medicine

Extracellular Recording of Neuronal Activity Combined with Microiontophoretic Application of Neuroactive Substances in Awake Mice

Differences in the activity of neurotransmitters and neuromodulators, and consequently different neural responses, can be found between anesthetized and awake animals. Therefore, methods allowing the manipulation of synaptic systems in awake animals are required in order to determine the contribution of synaptic inputs to neuronal processing unaffected by anesthetics. Here, we present methodology for the construction of electrodes to simultaneously record extracellular neural activity and release multiple neuroactive substances at the vicinity of the recording sites in awake mice. By combining these procedures, we performed microiontophoretic injections of gabazine to selectively block GABAA receptors in neurons of the inferior colliculus of head-restrained mice. Gabazine successfully modified neural response properties such as the frequency response area and stimulus-specific adaptation. Thus, we demonstrate that our methods are suitable for recording single-unit activity and for dissecting the role of specific neurotransmitter receptors in auditory processing.
The main limitation of the described procedure is the relatively short recording time (~3 hr), which is determined by the level of habituation of the animal to the recording sessions. On the other hand, multiple recording sessions can be performed in the same animal. The advantage of this technique over other experimental procedures used to manipulate the level of neurotransmission or neuromodulation (such as systemic injections or the use of optogenetic models), is that the drug effect is confined to the local synaptic inputs to the target neuron. In addition, the custom-manufacture of electrodes allows adjustment of specific parameters according to the neural structure and type of neuron of interest (such as the tip resistance for improving the signal-to-noise ratio of the recordings).

We present methods for the construction of electrodes to simultaneously record extracellular neural activity and release multiple neuroactive substances at the vicinity of the recording sites in awake mice. This technique allows the detailed analysis of putative local synaptic inputs to the neuron of interest.

Differences in the activity of neurotransmitters and neuromodulators, and consequently different neural responses, can be found between anesthetized and ...

Exposure of the Pig CNS for Histological Analysis: A Manual for Decapitation, Skull Opening, and Brain Removal

Pigs have become increasingly popular in large-animal translational neuroscience research as an economically and ethically feasible substitute to non-human primates. The large brain size of the pig allows the use of conventional clinical brain imagers and the direct use and testing of neurosurgical procedures and equipment from the human clinic. Further macroscopic and histological analysis, however, requires postmortem exposure of the pig central nervous system (CNS) and subsequent brain removal. This is not an easy task, as the pig CNS is encapsulated by a thick, bony skull and spinal column. The goal of this paper and instructional video is to describe how to expose and remove the postmortem pig brain and the pituitary gland in an intact state, suitable for subsequent macroscopic and histological analysis.

The goal of this paper and instructional video is to describe how to expose and remove the postmortem pig brain and pituitary gland in an intact state, suitable for subsequent macroscopic and histological analysis.

Pigs have become increasingly popular in large-animal translational neuroscience research as an economically and ethically feasible substitute to ...

Use of a Piglet Model for the Study of Anesthetic-induced Developmental Neurotoxicity (AIDN): A Translational Neuroscience Approach

Anesthesia cannot be avoided in many cases when surgery is required, particularly in children. Recent investigations in animals have raised concerns that anesthesia exposure may lead to neuronal apoptosis, known as anesthesia-induced developmental neurotoxicity (AIDN). Furthermore, some clinical studies in children have suggested that anesthesia exposure may lead to neurodevelopmental deficits later in life. Nonetheless, an ideal animal model for preclinical study has yet to be developed. The neonatal piglet represents a valuable model for preclinical study, as they share a striking number of developmental similarities with humans.
The anatomy and physiology of piglets allow for implementation of rigorous human perioperative conditions in both survival and non-survival procedures. Femoral artery catheterization allows for close monitoring, thus enabling prompt correction of any deviation of the piglet's vital signs and chemistries. In addition, there are multiple developmental similarities between piglets and human neonates. The techniques required to use piglets for experimentation will require experience to master. A pediatric anesthesiologist is a critical member of the investigative team. We describe, in a general sense, the appropriate use of a piglet model for neurodevelopmental study.

Use of a Piglet Model for the Study of Anesthetic-induced Developmental Neurotoxicity AIDN: A Translational Neuroscience Approach

Anesthesia-induced developmental neurotoxicity (AIDN) research has focused on rodents, which are not broadly applicable to humans. Non-human primate models are more relevant, but are cost-prohibitive and difficult to use for experimentation. The piglet, in contrast, is a clinically relevant, practical animal model ideal for the study of anesthetic neurotoxicity.

Anesthesia cannot be avoided in many cases when surgery is required, particularly in children.  Recent investigations in animals have raised concerns that ...

Noninvasive EEG Recordings from Freely Moving Piglets

The method allows the recording of high-quality electroencephalograms (EEGs) from freely moving piglets directly in the pigpen. We use a one-channel telemetric electroencephalography system in combination with standard self-adhesive hydrogel electrodes. The piglets are calmed down without the use of sedatives. After their release into the pigpen, the piglets behave normally&#8212;they drink and sleep in the same cycle as their siblings. Their sleep phases are used for the EEG recordings.

Here, we present a protocol to record telemetric electroencephalograms (EEGs) from freely moving piglets directly in the pigpen without the use of a sedative, making it possible to record typical EEG patterns during non-REM sleep, like spindle bursts.

The method allows the recording of high-quality electroencephalograms (EEGs) from freely moving piglets directly in the pigpen. We use a one-channel ...

Subdural Soft Electrocorticography (ECoG) Array Implantation and Long-Term Cortical Recording in Minipigs

Neurological impairments and diseases can be diagnosed or treated using electrocorticography (ECoG) arrays. In drug-resistant epilepsy, these help delineate the epileptic region to resect. In long-term applications such as brain-computer interfaces, these epicortical electrodes are used to record the movement intention of the brain, to control the robotic limbs of paralyzed patients. However, current stiff electrode grids do not answer the need for high-resolution brain recordings and long-term biointegration. Recently, conformable electrode arrays have been proposed to achieve long-term implant stability with high performance. However, preclinical studies for these new implant technologies are needed to validate their long-term functionality and safety profile for their translation to human patients. In this context, porcine models are routinely employed in developing medical devices due to their large organ sizes and easy animal handling. However, only a few brain applications are described in the literature, mostly due to surgery limitations and integration of the implant system on a living animal.
Here, we report the method for long-term implantation (6 months) and evaluation of soft ECoG arrays in the minipig model. The study first presents the implant system, consisting of a soft microfabricated electrode array integrated with a magnetic resonance imaging (MRI)-compatible polymeric transdermal port that houses instrumentation connectors for electrophysiology recordings. Then, the study describes the surgical procedure, from subdural implantation to animal recovery. We focus on the auditory cortex as an example target area where evoked potentials are induced by acoustic stimulation. We finally describe a data acquisition sequence that includes MRI of the whole brain, implant electrochemical characterization, intraoperative and freely moving electrophysiology, and immunohistochemistry staining of the extracted brains.
This model can be used to investigate the safety and function of novel design of cortical prostheses; mandatory preclinical study to envision translation to human patients.

Subdural Soft Electrocorticography ECoG Array Implantation and Long-Term Cortical Recording in Minipigs

Here, we present a method for the long-term performance and safety assessment of soft subdural electrode arrays in a minipig model, describing surgical method and tools, postoperative magnetic resonance imaging, electrophysiology of the auditory cortex, electrochemical properties of the implant, and postmortem immunochemistry.

Neurological impairments and diseases can be diagnosed or treated using electrocorticography (ECoG) arrays. In drug-resistant epilepsy, these help ...

Bioengineering

Angled Silicon Multielectrode Recordings for Deep Brainstem Structures in Mice

Acute Single-Unit Multi-Electrode Recordings from the Brainstem of Head-Fixed Mice

Silicon multielectrode-based recordings are increasingly popular for studying neuronal activity at the temporal resolution of action potentials in many brain regions. However, recording neuronal activity from deep caudal structures like the brainstem using multi-channel probes remains challenging. A significant concern is finding a trajectory for probe insertion that avoids large blood vessels, such as the superior sagittal venous sinus and the transverse venous sinus. Injuring these large veins can cause extensive bleeding, damage to the underlying brain tissue, and potentially death. This approach describes targeting brainstem structures by coupling anterior coordinates with an angled approach, allowing the recording probe to penetrate the brain below high-risk vascular structures. Compared to a strictly vertical approach, the angled approach maximizes the number of brain regions that can be targeted. Using this strategy, the ventrolateral periaqueductal gray (vlPAG), a brainstem region associated with REM sleep, can be reproducibly and reliably accessed to obtain single-unit, multi-electrode recordings in head-fixed mice before and during sevoflurane anesthesia. The ability to record neuronal activity in the vlPAG and surrounding nuclei with high temporal resolution is a step forward in advancing the understanding of the relationship between REM sleep and anesthesia.

Author Spotlight: Investigating Anesthesia-Induced Sleep Pathways and Neuronal Excitability in Mice

This protocol describes a method to obtain in vivo, high-density single-neuron recordings from the brainstem of head-fixed mice. This approach is deployed to measure the action potential firing of neurons in the ventrolateral periaqueductal gray - a brainstem region inactive during Rapid Eye Movement (REM) sleep - before and during general anesthesia.

Silicon multielectrode-based recordings are increasingly popular for studying neuronal activity at the temporal resolution of action potentials in many ...

Measuring Brain Glutamate Levels Under Anesthesia in Neonatal Piglets Using a Microelectrode Array

Source: Geyer, E. D., et al. <a href="https://app-jove-com.remotexs.ntu.edu.sg/v/57391">Adaptation of Microelectrode Array Technology for the Study of Anesthesia-induced Neurotoxicity in the Intact Piglet Brain.</a> J. Vis. Exp. (2018).
This video demonstrates the measurement of glutamate levels in the brain of an anesthetized neonatal piglet using a microelectrode array (MEA). The procedure involves creating a craniotomy window in the pig skull and inserting the MEA into the brain region of interest. The glutamate-oxidase-coated recording sites of the MEA convert extracellular brain glutamate to hydrogen peroxide, which generates a measurable current. This current is measured and normalized against background noise to determine brain glutamate levels under anesthesia.

All procedures involving animal models have been reviewed by the local institutional animal care committee and the JoVE veterinary review board.
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JoVE Encyclopedia of Experiments

Neurophysiology

Electrophysiology Techniques

Implanting a Wireless Bidirectional Microelectrode System in a Rat Brain

Source: Melo-Thomas, L., et al., <a href="https://app-jove-com.remotexs.ntu.edu.sg/v/56299">A Wireless, Bidirectional Interface for In Vivo Recording and Stimulation of Neural Activity in Freely Behaving Rats.</a> J. Vis. Exp. (2017)
The video demonstrates a procedure for implanting a wireless bidirectional multichannel electrode unit into a rat brain to record and stimulate multichannel neural networks.

Subdural Implantation of a Soft Electrocorticography Array for Cortical Electrophysiology Recording in Minipigs

Source: Fallegger, F. et al., <a href="https://app-jove-com.remotexs.ntu.edu.sg/v/64997">Subdural Soft Electrocorticography (ECoG) Array Implantation and Long-Term Cortical Recording in Minipigs.</a>&#160;J. Vis. Exp. (2023).
This video demonstrates the implantation of a soft electrocorticography array and the long-term cortical recordings in a minipig. It outlines the steps involved in surgically implanting the array over the minipig&#39;s auditory cortex and recording both baseline and sound stimulus-evoked neuronal action potentials.

Adaptation of Microelectrode Array Technology for the Study of Anesthesia-induced Neurotoxicity in the Intact Piglet Brain

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