The authors would like to thank the Hyde lab members for their thoughtful discussions, the Freimann Life Sciences Center technicians for zebrafish care and husbandry, and the University of Notre Dame Optical Microscopy Core/NDIIF for the use of instruments and their services. This work was supported by the Center for Zebrafish Research at the University of Notre Dame, the Center for Stem Cells and Regenerative Medicine at the University of Notre Dame, and grants from National Eye Institute of NIH R01-EY018417 (DRH), the National Science Foundation Graduate Research Fellowship Program (JTH), LTC Neil Hyland Fellowship of Notre Dame (JTH), Sentinels of Freedom Fellowship (JTH), and the Pat Tillman Scholarship (JTH).

Zebrafish were raised and maintained in the Notre Dame Zebrafish facility in the Freimann Life Sciences Center. The methods described in this manuscript were approved by the University of Notre Dame Animal Care and Use Committee.
1. Traumatic brain injury paradigm
<ol>
	<li>Add 1 mL of 2-phenoxyethanol to 1 L of system water (60 mg of Instant Ocean in 1 L of deionized RO water).</li>
	<li>Prepare an aerated recovery tank containing 2 L of system water at room temperature.</li>
	<li>Select the desired weight of ball bearing and a desired length and diameter of steel/plastic tubing and determine the energy and impact force. 
	NOTE: Tubing should have an inner diameter that allows the ball bearing to pass through without changing its path or speed of movement.
	<ol>
		<li>Determine the kinetic energy upon impact: 
		<img alt="Equation 1" src="/files/ftp_upload/62709/62709eq01.jpg" /> 
		Where, KE = kinetic energy, m = mass (in kg), g = gravitational force, h = height (in m) from drop point to fish. 
		NOTE: This provides kinetic energy in J. Multiply the value by 1,000 to determine mJ. KE is based on an accelerating object, which occurs when the ball bearing is dropped from a stationary position.</li>
		<li>Generate a mild TBI (miTBI) using 7.62 cm long steel/plastic tubing that ends 1.5 cm above the plate on the zebrafish skull (total distance 9.1 cm) and a 1.5 g (6.4 mm diameter) ball bearing. These produce a kinetic energy of 1.33 mJ. This damage was empirically decided to be equivalent to a miTBI based on key pathophysiological TBI markers, such as vascular injury, subdural/intracerebral hematoma formation, neuronal cell death, and cognitive impairments that largely recapitulated what was reported in the human population in a severity-dependent manner.</li>
		<li>Calculate kinetic energy miTBI = <img alt="Equation 2" src="/files/ftp_upload/62709/62709eq02.jpg" /></li>
		<li>Generate a moderate TBI (moTBI) using 12.7 cm long steel/plastic tubing that ends 1.5 cm above the plate on the zebrafish skull (total distance 14.2 cm) and a 1.5 g (6.4 mm diameter) ball bearing that produces kinetic energy of 2.08 mJ.</li>
		<li>Calculate kinetic energy moTBI = <img alt="Equation 3" src="/files/ftp_upload/62709/62709eq03.jpg" /></li>
		<li>Generate a severe TBI (sTBI) using 7.62 cm long steel/plastic tubing that ends 1.5 cm above the plate on the zebrafish skull (total distance 9.1 cm) and a 3.3 g (8.38 mm diameter) ball bearing that produces a kinetic energy of 2.94 mJ.</li>
		<li>Calculate kinetic energy sTBI =&#160; <img alt="Equation 4" src="/files/ftp_upload/62709/62709eq04.jpg" /></li>
	</ol>
	</li>
	<li>Fill a Petri dish with modeling clay (Figure 1, step 1) and use a blunt instrument (i.e., the back of a pair of forceps) to create a raised platform (5 cm x 1.5 cm) with additional modeling clay (Figure 1, step 2).
	<ol>
		<li>Use a razor blade to divide the raised platform lengthwise into two approximately equal halves (Figure 1, step 3, red dashed line). Form the two halves into a channel that accommodates the length of an adult fish (Figure 1, step 4). Use additional clay to build walls that will secure ~2/3 of the fish body, leaving the head exposed.</li>
		<li>Mold a small support in the exposed head region perpendicular to the walls to support the head to avoid rotation or recoil of the head upon injury (Figure 1, step 4). 
		NOTE: The channel should be deep enough to support the fish in a dorsal-up position but should still allow the head to rest above the surrounding clay. Additionally, the head support should follow the natural curvature of the fish, supporting the lower mandible and gills.</li>
		<li>Ensure that the dropped weight is not impeded by the channel&#39;s sides (Figure 1, step 4).</li>
	</ol>
	</li>
	<li>Create a 3 mm diameter steel disk using a mini hole-punch and 22 g steel flashing. Each disk may be used multiple times.</li>
	<li>Anesthetize one fish by placing it into a beaker with 50-100 mL of 1:1000 (1 mL/1 L, 0.1%) 2-phenoxyethanol until it is unresponsive to tail pinch.</li>
	<li>Place the fish, dorsal side up, on the clay mold within the channel so that the body is secured on the sides and place a 3 mm 22 g steel disc on the head, centered over the desired impact point (Figure 1, step 5).
	<ol>
		<li>Ensure that the fish is aligned as perpendicularly as possible to avoid its head from tilting to one side, which could cause an uneven impact.</li>
	</ol>
	</li>
	<li>Secure the steel/plastic tubing, using a standard ring stand and arm clamp, so the bottom of the tubing is 1.5 cm above the head of the zebrafish (Figure 1, step 6). Ensure the tubing is straight.
	<ol>
		<li>Look down the tubing and ensure that the tubing is aligned above the steel plate.</li>
	</ol>
	</li>
	<li>Drop the ball bearing (1.5 g for mild and moderate TBI, and 3.3 g for severe TBI) from a predetermined height (described in Steps 1.3.3-1.3.5) down the tubing onto the steel plate located over the desired neuroanatomical region of interest (e.g., cerebellum, Figure 1, step 5) to produce the blunt-force TBI for the desired severity of injury. Place the injured fish in a recovery tank to be monitored. 
	NOTE: Depending on the severity of the injury, mortality or tonic-clonic seizures may occur. If the fish are unresponsive for a prolonged period of time following the TBI, use a transfer pipette or forceps to administer a tail-pinch and evaluate for a pain response.</li>
</ol>
2. Scoring seizures post-TBI in the adult zebrafish
<ol>
	<li>Anesthetize and injure the fish according to the injury protocol outlined in section 1 and place the injured fish in an aerated recovery tank of 2 L of system water.</li>
	<li>Observe the fish for any signs of post-traumatic seizures beginning immediately after being placed in the recovery tank. Set an observation time (i.e., 1 h) and record all seizure activity, including the seizure score (described below), duration of each seizure, and the percentage of fish that experienced seizures (Figure 2A). 
	NOTE: Seizures can occur immediately upon injury, as well as hours or days post-TBI. Seizures can persist long term and a single fish can have multiple seizures. Setting an observation time of 1 h or greater will yield a good representation of the overall trend of seizure rates.</li>
	<li>Score fish using the Mussulini18 guidelines for adult zebrafish seizure phenotypes. 
	&#8203;NOTE: Without using the tracking software, it is difficult to assess seizure scores below 3 unbiasedly. Therefore, only seizure scores of 3 or greater should be recorded when the assessment is being performed without software.</li>
</ol>
3. Brain dissection
<ol>
	<li>Euthanize fish in a 1:500 (2 mL/1 L, 0.2%) solution of 2-phenoxyethanol, until gill movements cease, and they are unreactive to fin pinch, at the desired endpoint.</li>
	<li>Fill a Petri dish with modeling clay and create a small cavity to support the body during dissection.</li>
	<li>Place the fish, dorsal side up, in the clay mold. Place one dissection pin through the midline halfway down the body of the fish and a second pin ~5 mm behind the base of the head.</li>
	<li>Under a dissecting light microscope, bluntly sever the optic nerve with a pair of #5 Dumont forceps and remove the eyes (Figure 2A).</li>
	<li>Orientate the fish so that the rostral end is furthest when looking through the microscope (Figure 2B). 
	NOTE: The following steps are for right-handed individuals. Left-handed individuals may prefer to perform the following steps in a mirrored orientation.</li>
	<li>Use #5 forceps to slowly place one end of the forceps under the right parietal plate, making a deliberate scissor action moving toward the rostral end and remove the right parietal and frontal plates (Figure 2C).
	<ol>
		<li>Keep the forceps at an angle of 45&#176; or lower in order to avoid penetrating the brain during dissection.</li>
	</ol>
	</li>
	<li>Rotate the fish 90&#730; clockwise. Place one end of the #5 forceps under the left parietal plate and use the same scissor motion to remove the left parietal and frontal plates exposing the entire dorsal aspect of the brain (Figure 2D,E).</li>
	<li>Bluntly transect the maxilla with #5 forceps. Preserve the olfactory bulbs and do not damage them if this is the region of interest.</li>
	<li>Remove the right opercle, preopercle, interopercle, and subopercle with #5 forceps (Figure 2F).</li>
	<li>Bluntly resect the musculature at the caudal end of the calvarium opening using #5 forceps, exposing the spinal cord.</li>
	<li>Bluntly transect the spinal cord with #5 forceps. Carefully place forceps under the brain and gently remove the brain from the calvarium. 
	NOTE: Never pinch the brain. Use forceps to &#34;cradle&#34; the brain or resect caudally and utilize the exposed spinal cord as a pinch point to maneuver the brain.</li>
	<li>Fix the removed brains in 9 parts 100% ethanol to 1 part 37% formaldehyde overnight at 4&#176;C on a rocker platform.</li>
</ol>
4. Edema studies in the zebrafish brain
<ol>
	<li>Anesthetize and injure fish according to the injury protocol outlined in section 1 and allow the fish to recover in a recovery tank until they start swimming freely.</li>
	<li>Place fish back in the normal housing conditions post-injury for 1 day.</li>
	<li>Euthanize the fish in 1:500 2-phenoxyethanol, after time has elapsed.</li>
	<li>Dissect the whole brain or region of interest according to the protocol outlined in section 3 and place the brain immediately on a small weigh boat. 
	NOTE: Use caution when transferring the brain, using fine forceps to gently place it on the weigh boat without stabbing or scraping the brain, which could result in the loss of tissue.</li>
	<li>Label (with injury group and brain number) and tare an additional small drying weigh boat on a scale. Use a scale with the ability to measure a minimum of 0.001 g to get an accurate measurement.</li>
	<li>Transfer the brain to the tared drying weigh boat and record the wet weight of the brain. Orient the brains so that they lay flat on the weigh boat with the dorsal side facing up.</li>
	<li>Place the drying weigh boat and brain in a hybridization oven set to 60 &#176;C for 8 h.</li>
	<li>After drying, the brain may stick to the drying weigh boat and may be difficult to remove and transfer to a new tared small weigh boat. Avoid pinching the brain with forceps, as this might result in damage to the dry brain and loss of tissue. Instead, pinch the fine forceps together and, starting at the ventral side of the brain, scoop in an upward motion.</li>
	<li>Determine the water content of each brain using the formula (Figure 4): 
	<img alt="Equation 5" src="/files/ftp_upload/62709/62709eq05.jpg" /></li>
</ol>
5. Labeling cellular proliferation across the neuroaxis and preparing fixed tissue.
<ol>
	<li>Prepare 10 mM 5-ethynyl-2&#39;-deoxyuridine (EdU) in 2 mL of ddH2O.</li>
	<li>Anesthetize 3 to 4 fish at a time in 50-100 mL of 1:1000 (1 mL/1 L, 0.1%) 2-phenoxyethanol until the fish are unresponsive to tail pinch, at the desired time point following injury (using the protocol outlined in section 1).</li>
	<li>Make a partial incision on a wet sponge and place one fish at a time in the opening, ventral side up.</li>
	<li>Use a 30 G needle to inject ~40 &#181;L of 10 mM EdU into the fish&#39;s body. Return the fish to a holding tank filled with system water. 
	NOTE: Repeated injections may be performed at different time points to label a greater number of proliferating cells and may be needed if a chase period of greater than 1 week is desired.</li>
	<li>Collect brains as outlined in section 3 and place them as a group in a 5 mL glass vial containing 2 mL of 9 parts 100% ethanol to 1 part 37% formaldehyde. Fix the brains at 4 &#176;C on a rocker platform. 
	NOTE: A rocker or shaker platform prohibits the brains from resting at the bottom and the telencephalon of whole brains from curling.</li>
	<li>Rehydrate brains, in the same glass vial used to fix brains, in washes of descending ethanol series, 75%, 50%, and 25%, for 15 mins each, followed by a 1.5 h wash in 5% sucrose/PBS on a rocker at room temperature. Store the brains in a glass vial overnight in 30% sucrose/PBS at 4&#176; C on a rocker platform.</li>
	<li>Remove brains from 30% sucrose/PBS and transfer them with forceps into a 12-well plate (one treatment group per well) with wells filled with a 2:1 solution consisting of 2 parts tissue freezing medium and 1 part 30% sucrose/PBS. Incubate the brains overnight at 4 &#176;C on a rocker platform.</li>
	<li>Transfer brains to the next row of wells within the 12-well plate submerging brains in 100% TFM for 2-24 h at 4 &#176;C.</li>
	<li>Use a cryostat chuck to embed the brains in TFM in the desired orientation on dry ice.</li>
	<li>Perform cryosectioning (16 &#956;m thick sections) and collect the sections on positively charged slides. Dry slides on a slide warmer for 1 h and then store at -80 &#176;C or continue with immunohistochemistry.</li>
	<li>Prepare a hydrophobic barrier on the slide around the tissue sections and allow to dry on a slide warmer for 20 min.</li>
	<li>Briefly wash the slides in PBS for 5 min and then twice in PBS-Tween 20 (0.05%) for 10 min each.</li>
	<li>Perform EdU detection using the EdU Cell Proliferation Kit and the manufacturer&#39;s instructions.</li>
	<li>Analyze the slides and quantify the fluorescent EdU-labeled cells using either an epifluorescent microscope or a confocal microscope. A minimum of a 40x objective will be required to clearly distinguish individual cells.</li>
</ol>

<ol>
	<li>Centers for Disease Control and Prevention. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Surveillance+Report+of+Traumatic+Brain+Injury-related+Emergency+Department+Visits,+Hospitalizations,+and+Deaths-United+States,+2014.">Surveillance Report of Traumatic Brain Injury-related Emergency Department Visits, Hospitalizations, and Deaths-United States, 2014.</a> Centers for Disease Control and Prevention, U.S. Department of Health and Human Services. , (2019).</li><li>Galgano, M., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Traumatic+brain+injury:+current+treatment+strategies+and+future+endeavors.">Traumatic brain injury: current treatment strategies and future endeavors.</a> Cell transplantation. 26 (7), 1118-1130 (2017).</li><li>Santiago, L. A., Oh, B. C., Dash, P. K., Holcomb, J. B., Wade, C. E. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+clinical+comparison+of+penetrating+and+blunt+traumatic+brain+injuries.">A clinical comparison of penetrating and blunt traumatic brain injuries.</a> Brain injury. 26 (2), 107-125 (2012).</li><li>Korley, F. K., Kelen, G. D., Jones, C. M., Diaz-Arrastia, R. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Emergency+department+evaluation+of+traumatic+brain+injury+in+the+United+States,+2009-2010.">Emergency department evaluation of traumatic brain injury in the United States, 2009-2010.</a> The Journal of Head Trauma Rehabilitation. 31 (6), 379-387 (2016).</li><li>Faul, M., Xu, L., Wald, M., Coronado, V. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=.">.</a> Traumatic Brain Injury in the United States: Emergency Department Visits, Hospitalizations and Deaths. , (2010).</li><li>Campbell, L. J., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Notch3+and+DeltaB+maintain+M&#252;ller+glia+quiescence+and+act+as+negative+regulators+of+regeneration+in+the+light-damaged+zebrafish+retina.">Notch3 and DeltaB maintain M&#252;ller glia quiescence and act as negative regulators of regeneration in the light-damaged zebrafish retina.</a> Glia. 69 (3), 546-566 (2021).</li><li>Green, L. A., Nebiolo, J. C., Smith, C. J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Microglia+exit+the+CNS+in+spinal+root+avulsion.">Microglia exit the CNS in spinal root avulsion.</a> PLoS Biology. 17 (2), 3000159 (2019).</li><li>Hentig, J., Byrd-Jacobs, C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Exposure+to+zinc+sulfate+results+in+differential+effects+on+olfactory+sensory+neuron+subtypes+in+the+adult+zebrafish.">Exposure to zinc sulfate results in differential effects on olfactory sensory neuron subtypes in the adult zebrafish.</a> International Journal of Molecular Sciences. 17 (9), 1445 (2016).</li><li>Ito, Y., Tanaka, H., Okamoto, H., Oshima, T. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Characterization+of+neural+stem+cells+and+their+progeny+in+the+adult+zebrafish+optic+tectum.">Characterization of neural stem cells and their progeny in the adult zebrafish optic tectum.</a> Developmental Biology. 342 (1), 26-38 (2010).</li><li>Becker, C., Becker, T. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Adult+zebrafish+as+a+model+for+successful+central+nervous+system+regeneration.">Adult zebrafish as a model for successful central nervous system regeneration.</a> Restorative Neurology and Neuroscience. 26 (2-3), 71-80 (2008).</li><li>Alyenbawwi, H., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Seizures+are+a+druggable+mechanistic+link+between+TBI+and+subsequent+tauopathy.">Seizures are a druggable mechanistic link between TBI and subsequent tauopathy.</a> eLife. 10, 58744 (2021).</li><li>Kaslin, J., Kroehne, V., Ganz, J., Hans, S., Brand, M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Distinct+roles+of+neuroepithelia-like+and+radial+glia-like+progenitor+cells+in+cerebellar+regeneration.">Distinct roles of neuroepithelia-like and radial glia-like progenitor cells in cerebellar regeneration.</a> Development. 144 (8), 1462-1471 (2017).</li><li>McCutcheon, V., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+novel+model+of+traumatic+brain+injury+in+adult+zebrafish+demonstrates+response+to+injury+and+treatment+comparable+with+mammalian+models.">A novel model of traumatic brain injury in adult zebrafish demonstrates response to injury and treatment comparable with mammalian models.</a> Journal of Neurotrauma. 34 (7), 1382-1393 (2017).</li><li>Skaggs, K., Goldman, D., Parent, J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Excitotoxic+brain+injury+in+adult+zebrafish+stimulates+neurogenesis+and+long-distance+neuronal+integration.">Excitotoxic brain injury in adult zebrafish stimulates neurogenesis and long-distance neuronal integration.</a> Glia. 62 (12), 2061-2079 (2014).</li><li>Kishimoto, N., Shimizu, K., Sawamoto, K. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Neuronal+regeneration+in+a+zebrafish+model+of+adult+brain+injury.">Neuronal regeneration in a zebrafish model of adult brain injury.</a> Disease Models &amp; Mechanisms. 5 (2), 200-209 (2012).</li><li>Kroehne, V., Freudenreich, D., Hans, S., Kaslin, J., Brand, M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Regeneration+of+the+adult+zebrafish+brain+from+neurogenic+radial+glia-type+progenitors.">Regeneration of the adult zebrafish brain from neurogenic radial glia-type progenitors.</a> Development. 138 (22), 4831-4841 (2011).</li><li>Marmarou, A., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+new+model+of+diffuse+brain+injury+in+rats.+Part+I:+Pathophysiology+and+biomechanics.">A new model of diffuse brain injury in rats. Part I: Pathophysiology and biomechanics.</a> Journal of Neurosurgery. 80 (2), 291-300 (1994).</li><li>Mussulini, B. H., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Seizures+induced+by+pentylenetetrazole+in+the+adult+zebrafish:+a+detailed+behavioral+characterization.">Seizures induced by pentylenetetrazole in the adult zebrafish: a detailed behavioral characterization.</a> PloS One. 8 (1), 54515 (2013).</li><li>Kalueff, A., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Towards+a+comprehensive+catalog+of+zebrafish+behavior+1.0+and+beyond.">Towards a comprehensive catalog of zebrafish behavior 1.0 and beyond.</a> Zebrafish. 10 (1), 70-86 (2013).</li><li>Xiong, Y., Mahmood, A., Chopp, M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Animal+models+of+traumatic+brain+injuries.">Animal models of traumatic brain injuries.</a> Nature Reviews Neuroscience. 14, 128-142 (2013).</li><li>Amamoto, R., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Adult+axolotls+can+regenerate+original+neuronal+diversity+in+response+to+brain+injury.">Adult axolotls can regenerate original neuronal diversity in response to brain injury.</a> eLife. 5, 13998 (2016).</li><li>Yamamoto, S., Levin, H., Prough, D. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Mild,+moderate+and+severe:+terminology+implications+for+clinical+and+experimental+traumatic+brain+injury.">Mild, moderate and severe: terminology implications for clinical and experimental traumatic brain injury.</a> Current Opinion in Neurology. 31 (6), 672-680 (2008).</li><li>Lund, S., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Moderate+traumatic+brain+injury,+acute+phase+course+and+deviations+in+physiological+variables:+an+observational+study.">Moderate traumatic brain injury, acute phase course and deviations in physiological variables: an observational study.</a> Scandinavian Journal of Trauma Resuscitation and Emergency Medicine. 24, 77 (2016).</li><li>Levin, H., Arrastia, R. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Diagnosis,+prognosis,+and+clinical+management+of+mild+traumatic+brain+injury.">Diagnosis, prognosis, and clinical management of mild traumatic brain injury.</a> The Lancet Neurology. 14 (5), 506-517 (2015).</li><li>Ruff, R. M., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Recommendations+for+diagnosing+a+mild+traumatic+brain+injury:+a+National+Academy+of+Neuropsychology+education+paper.">Recommendations for diagnosing a mild traumatic brain injury: a National Academy of Neuropsychology education paper.</a> Archives of Clinical Neuropsychology: The Official Journal of the National Academy of Neuropsychologists. 24 (1), 3-10 (2009).</li><li>Ganz, J., Brand, M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Adult+neurogenesis+in+fish.">Adult neurogenesis in fish.</a> Cold Spring Harbor Perspectives in Biology. 8 (7), 019018 (2016).</li><li>Grandel, H., Kaslin, J., Ganz, J., Wenzel, I., Brand, M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Neural+stem+cells+and+neurogenesis+in+the+adult+zebrafish+brain:+origin,+proliferation+dynamics,+migration+and+cell+fate.">Neural stem cells and neurogenesis in the adult zebrafish brain: origin, proliferation dynamics, migration and cell fate.</a> Developmental Biology. 295, 263-277 (2006).</li><li>Lahne, M., Nagashima, M., Hyde, D. R., Hitchcock, P. F. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Reprogramming+Muller+glia+to+regenerate+retinal+neurons.">Reprogramming Muller glia to regenerate retinal neurons.</a> Annual Review of Visual Science. 6, 171-193 (2020).</li></ol>

The authors have nothing to disclose.

Investigations of neurotrauma and associated sequelae have long been centered on traditional non-regenerative rodent models20. Only recently have studies applied various forms of CNS damage to regenerative models9,11,13,14,21. Though insightful, these models are limited by either their use of an injury method uncommonly seen in the huma...

Traumatic brain injuries (TBIs) are a global health crisis and a leading cause of death and disability. In the United States, approximately 2.9 million people experience a TBI each year, and between 2006-2014 mortality due to TBI or TBI sequelae increased by over 50%1. However, TBIs vary in their etiology, pathology, and clinical presentation due largely in part to the mechanism of injury (MOI), which also influences treatment strategies and predicted prognosis2. Though TBIs can result from various MOI, they are predominately the result of either a penetrating or blunt-force trauma. Penetrating traumas represent a small percentage of TBIs and generate a severe and focal injury that is localized to the immediate and surrounding impaled brain regions3. In contrast, blunt-force TBIs are more common in the general population, span a range of severities (mild, moderate, and severe), and produce a diffuse, heterogeneous, and global injury affecting multiple brain regions1,4,5.
Zebrafish (Danio rerio) have been utilized to examine a wide range of neurological insults spanning the central nervous system (CNS)6,7,8,9. Zebrafish also possess, unlike mammals, an innate and robust regenerative response to repair CNS damage10. Current zebrafish trauma models use various injury methods, including penetration, excision, chemical insult, or pressure waves11,12,13,14,15,16. However, each of these methods utilizes an MOI that is rarely experienced by the human population, is not scalable across a range of injury severities, and does not address the heterogeneity or severity-dependent TBI sequela reported after blunt-force TBI. These factors limit the use of the zebrafish model to understand the underlying mechanisms of the pathologies associated with the most common form of TBI in the human population (mild blunt-force injuries).
We aimed to develop a rapid and scalable blunt-force TBI zebrafish model that provides avenues to investigate injury pathology, progression of TBI sequela, and the innate regenerative response. We modified the commonly used rodent Marmarou17 weight drop and applied it to adult zebrafish. This model yields a reproducible range of severities ranging from mild, moderate, to severe. This model also recapitulates multiple facets of human TBI pathology, in a severity-dependent manner, including seizures, edema, subdural and intracerebral hematomas, neuronal cell death, and cognitive deficits, such as learning and memory impairment. Days following injury, pathologies and deficits dissipate, returning to levels resembling undamaged controls. Additionally, this zebrafish model displays a robust proliferation and neuronal regeneration response across the neuroaxis concerning injury severity.
Here, we provide details toward the set up and induction of blunt-force trauma, scoring post-traumatic seizures, assessment of vascular injuries, instructions on preparing brain sections, approaches to quantifying edema, and insight into the proliferative response following injury.

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>2-phenoxyethanol</td>
			<td>Sigma Alderich</td>
			<td>77699</td>
			<td></td>
		</tr>
		<tr>
			<td>#00 buckshot</td>
			<td>Remington</td>
			<td>RMS23770</td>
			<td>3.3g weight for sTBI</td>
		</tr>
		<tr>
			<td>#3 buckshot</td>
			<td>Remington</td>
			<td>RMS23776</td>
			<td>1.5g weight for miTBI/moTBI</td>
		</tr>
		<tr>
			<td>#5 Dumont forceps</td>
			<td>WPI</td>
			<td>14098</td>
			<td></td>
		</tr>
		<tr>
			<td>5-ethynyl-2&#8217;-deoxyuridine</td>
			<td>Life Technologies</td>
			<td>A10044</td>
			<td>EdU</td>
		</tr>
		<tr>
			<td>5ml glass vial</td>
			<td>VWR</td>
			<td>66011-063</td>
			<td></td>
		</tr>
		<tr>
			<td>Click-iT EdU Cell Proliferation Kit</td>
			<td>Life Technologies</td>
			<td>C10340</td>
			<td></td>
		</tr>
		<tr>
			<td>CytoOne 12-well plate</td>
			<td>USA Scientific</td>
			<td>CC7682-7512</td>
			<td></td>
		</tr>
		<tr>
			<td>Instant Ocean</td>
			<td>Instant Ocean</td>
			<td>SS15-10</td>
			<td></td>
		</tr>
		<tr>
			<td>Super frost postiviely charged slides</td>
			<td>VWR</td>
			<td>48311-703</td>
			<td></td>
		</tr>
		<tr>
			<td>Super PAP Pen Liquid Blocker</td>
			<td>Ted Pella</td>
			<td>22309</td>
			<td></td>
		</tr>
		<tr>
			<td>Tissue freezing medium</td>
			<td>VWR</td>
			<td>15148-031</td>
			<td></td>
		</tr>
	</tbody>
</table>

a scalable model to study the effects of blunt-force injury in adult zebrafish

Blunt-force traumatic brain injuries (TBI) are the most common form of head trauma, which spans a range of severities and results in complex and heterogenous secondary effects. While there is no mechanism to replace or regenerate the lost neurons following a TBI in humans, zebrafish possess the ability to regenerate neurons throughout their body, including the brain. To examine the breadth of pathologies exhibited in zebrafish following a blunt-force TBI and to study the mechanisms underlying the subsequent neuronal regenerative response, we modified the commonly used rodent Marmarou weight drop for the use in adult zebrafish. Our simple blunt-force TBI model is scalable, inducing a mild, moderate, or severe TBI, and recapitulates many of the phenotypes observed following human TBI, such as contact- and post-traumatic seizures, edema, subdural and intracerebral hematomas, and cognitive impairments, each displayed in an injury severity-dependent manner. TBI sequelae, which begin to appear within minutes of the injury, subside and return to near undamaged control levels within 7 days post-injury. The regenerative process begins as early as 48 hours post-injury (hpi), with the peak cell proliferation observed by 60 hpi. Thus, our zebrafish blunt-force TBI model produces characteristic primary and secondary injury TBI pathologies similar to human TBI, which allows for investigating disease onset and progression, along with the mechanisms of neuronal regeneration that is unique to zebrafish.

Preparing the injury-induction rig allows for a rapid and simplistic means of delivering a scalable blunt-force TBI to adult zebrafish. The graded severity of the injury model provides several easily identifiable metrics of successful injury, though the vascular injury is one of the easiest and most prominent pathologies (Figure 3). The strain of fish used during the injury can make this indicator easier or harder to identify. When using wild-type AB fish(WTAB, <...

Watch this Scientific Journal Video about A Scalable Model to Study the Effects of Blunt-Force Injury in Adult Zebrafish at JoVE.com

A Scalable Model to Study the Effects of Blunt-Force Injury in Adult Zebrafish

We modified the Marmarou weight drop model for adult zebrafish to examine a breadth of pathologies following blunt-force traumatic brain injury (TBI) and the mechanisms underlying subsequent neuronal regeneration. This blunt-force TBI model is scalable, induces a mild, moderate, or severe TBI, and recapitulates injury heterogeneity observed in human TBI.

Blunt-force traumatic brain injuries (TBI) are the most common form of head trauma, which spans a range of severities and results in complex and ...

a-scalable-model-to-study-effects-blunt-force-injury-adult

Research

JoVE Journal

Neuroscience

3.2K Views.  University of Notre Dame. We modified the Marmarou weight drop model for adult zebrafish to examine a breadth of pathologies following blunt-force traumatic brain injury (TBI) and the mechanisms underlying subsequent neuronal regeneration. This blunt-force TBI model is scalable, induces a mild, moderate, or severe TBI, and recapitulates injury heterogeneity observed in human TBI.

Video: A Scalable Model to Study the Effects of Blunt-Force Injury in Adult Zebrafish

An Optic Nerve Crush Injury Murine Model to Study Retinal Ganglion Cell Survival

Injury to the optic nerve can lead to axonal degeneration, followed by a gradual death of retinal ganglion cells (RGCs), which results in irreversible vision loss. Examples of such diseases in human include traumatic optic neuropathy and optic nerve degeneration in glaucoma. It is characterized by typical changes in the optic nerve head, progressive optic nerve degeneration, and loss of retinal ganglion cells, if uncontrolled, leading to vision loss and blindness.
The optic nerve crush (ONC) injury mouse model is an important experimental disease model for traumatic optic neuropathy, glaucoma, etc. In this model, the crush injury to the optic nerve leads to gradual retinal ganglion cells apoptosis. This disease model can be used to study the general processes and mechanisms of neuronal death and survival, which is essential for the development of therapeutic measures. In addition, pharmacological and molecular approaches can be used in this model to identify and test potential therapeutic reagents to treat different types of optic neuropathy.
Here, we provide a step by step demonstration of (I) Baseline retrograde labeling of retinal ganglion cells (RGCs) at day 1, (II) Optic nerve crush injury at day 4, (III) Harvest the retinae and analyze RGC survival at day 11, and (IV) Representative result.

This protocol shows how to retrogradely label retinal ganglion cells, and how to subsequently make an optic nerve crush injury in order to analyze retinal ganglion cell survival and apoptosis. It is an experimental disease model for different types of optic neuropathy, including glaucoma.

Injury to the optic nerve can lead to axonal degeneration, followed by a gradual death of retinal ganglion cells (RGCs), which results in irreversible ...

Micromanipulation of Gene Expression in the Adult Zebrafish Brain Using Cerebroventricular Microinjection of Morpholino Oligonucleotides

Manipulation of gene expression in tissues is required to perform functional studies. In this paper, we demonstrate the cerebroventricular microinjection (CVMI) technique as a means to modulate gene expression in the adult zebrafish brain. By using CVMI, substances can be administered into the cerebroventricular fluid and be thoroughly distributed along the rostrocaudal axis of the brain. We particularly focus on the use of antisense morpholino oligonucleotides, which are potent tools for knocking down gene expression in vivo. In our method, when applied, morpholino molecules are taken up by the cells lining the ventricular surface. These cells include the radial glial cells, which act as neurogenic progenitors. Therefore, knocking down gene expression in the radial glial cells is of utmost importance to analyze the widespread neurogenesis response in zebrafish, and also would provide insight into how vertebrates could sustain adult neurogenesis response. Such an understanding would also help the efforts for clinical applications in human neurodegenerative disorders and central nervous system regeneration. Thus, we present the cerebroventricular microinjection method as a quick and efficient way to alter gene expression and neurogenesis response in the adult zebrafish forebrain. We also provide troubleshooting tips and other useful information on how to carry out the CVMI procedure.

In this article, we demonstrate a method for manipulation of gene expression in the ventricular cells of the adult zebrafish telencephalon using antisense morpholino oligonucleotides. We present this method as an efficient and quick protocol that can be used for functional studies in the adult vertebrate brain.

Manipulation of gene expression in tissues is  required to perform functional studies. In this paper, we demonstrate the  cerebroventricular ...

Electrophysiological Recording in the Brain of Intact Adult Zebrafish

Previously, electrophysiological studies in adult zebrafish have been limited to slice preparations or to eye cup preparations and electrorentinogram recordings. This paper describes how an adult zebrafish can be immobilized, intubated, and used for in vivo electrophysiological experiments, allowing recording of neural activity. Immobilization of the adult requires a mechanism to deliver dissolved oxygen to the gills in lieu of buccal and opercular movement. With our technique, animals are immobilized and perfused with habitat water to fulfill this requirement. A craniotomy is performed under tricaine methanesulfonate (MS-222; tricaine) anesthesia to provide access to the brain. The primary electrode is then positioned within the craniotomy window to record extracellular brain activity. Through the use of a multitube perfusion system, a variety of pharmacological compounds can be administered to the adult fish and any alterations in the neural activity can be observed. The methodology not only allows for observations to be made regarding changes in neurological activity, but it also allows for comparisons to be made between larval and adult zebrafish. This gives researchers the ability to identify the alterations in neurological activity due to the introduction of various compounds at different life stages.

This paper describes how an adult zebrafish can be immobilized, intubated, and used for in vivo electrophysiological experiments to allow recordings and manipulation of neural activity in an intact animal.

Previously, electrophysiological studies in adult zebrafish have been limited to slice preparations or to eye cup preparations and electrorentinogram ...

Stab Wound Injury of the Zebrafish Adult Telencephalon: A Method to Investigate Vertebrate Brain Neurogenesis and Regeneration

Adult zebrafish have an amazing capacity to regenerate their central nervous system after injury. To investigate the cellular response and the molecular mechanisms involved in zebrafish adult central nervous system (CNS) regeneration and repair, we developed a zebrafish model of adult telencephalic injury.
In this approach, we manually generate an injury by pushing an insulin syringe needle into the zebrafish adult telencephalon. At different post injury days, fish are sacrificed, their brains are dissected out and stained by immunohistochemistry and/or in situ hybridization (ISH) with appropriate markers to observe cell proliferation, gliogenesis, and neurogenesis. The contralateral unlesioned hemisphere serves as an internal control. This method combined for example with RNA deep sequencing can help to screen for new genes with a role in zebrafish adult telencephalon neurogenesis, regeneration, and repair.

To shed light on the cellular and molecular mechanisms of zebrafish adult neurogenesis and regeneration, we developed a protocol for invasive surgery causing mechanical injuries in the zebrafish adult telencephalon and subsequent monitoring of changes in the stabbed hemisphere by immunohistochemistry or in situ hybridization.

Adult zebrafish have an amazing capacity to regenerate their central nervous system after injury. To investigate the cellular response and the molecular ...

The Olfactory System as a Model to Study Axonal Growth Patterns and Morphology In Vivo

The olfactory system has the unusual capacity to generate new neurons throughout the lifetime of an organism. Olfactory stem cells in the basal portion of the olfactory epithelium continuously give rise to new sensory neurons that extend their axons into the olfactory bulb, where they face the challenge to integrate into existing circuitry. Because of this particular feature, the olfactory system represents a unique opportunity to monitor axonal wiring and guidance, and to investigate synapse formation. Here we describe a procedure for in vivo labeling of sensory neurons and subsequent visualization of axons in the olfactory system of larvae of the amphibian Xenopus laevis. To stain sensory neurons in the olfactory organ we adopt the electroporation technique. In vivo electroporation is an established technique for delivering fluorophore-coupled dextrans or other macromolecules into living cells. Stained sensory neurons and their axonal processes can then be monitored in the living animal either using confocal laser-scanning or multiphoton microscopy. By reducing the number of labeled cells to few or single cells per animal, single axons can be tracked into the olfactory bulb and their morphological changes can be monitored over weeks by conducting series of in vivo time lapse imaging experiments. While the described protocol exemplifies the labeling and monitoring of olfactory sensory neurons, it can also be adopted to other cell types within the olfactory and other systems.

The Olfactory System as a Model to Study Axonal Growth Patterns and Morphology In Vivo

We describe a protocol for in vivo labeling of olfactory sensory neurons by electroporation and subsequent confocal laser-scanning or multiphoton microscopy to visualize neuronal morphology and its development over time.

The olfactory system has the unusual capacity to generate new neurons throughout the lifetime of an organism. Olfactory stem cells in the basal portion of ...

A Simple One-step Dissection Protocol for Whole-mount Preparation of Adult Drosophila Brains

There is an increasing interest in using Drosophila to model human brain degenerative diseases, map neuronal circuitries in adult brains, and study the molecular and cellular basis of higher brain functions. A whole-mount preparation of adult brains with well-preserved morphology is critical for such whole brain-based studies, but can be technically challenging and time-consuming. This protocol describes an easy-to-learn, one-step dissection approach of an adult fly head in less than 10 s, while keeping the intact brain attached to the rest of the body to facilitate subsequent processing steps. The procedure helps remove most of the eye and tracheal tissues normally associated with the brain that can interfere with the later imaging step, and also places less demand on the quality of the dissecting forceps. Additionally, we describe a simple method that allows convenient flipping of the mounted brain samples on a coverslip, which is important for imaging both sides of the brains with similar signal intensity and quality. As an example of the protocol, we present an analysis of dopaminergic (DA) neurons in adult brains of WT (w1118) flies. The high efficacy of the dissection method makes it particularly useful for large-scale adult brain-based studies in Drosophila.

A Simple One-step Dissection Protocol for Whole-mount Preparation of Adult Drosophila Brains

The adult Drosophila brain is a valuable system for studying neuronal circuitry, higher brain functions, and complex disorders. An efficient method to dissect whole brain tissue from the small fly head will facilitate brain-based studies. Here we describe a simple, one-step dissection protocol of adult brains with well-preserved morphology.

There is an increasing interest in using Drosophila to model human brain degenerative diseases, map neuronal circuitries in adult brains, and study the ...

Effects of Blast-induced Neurotrauma on Pressurized Rodent Middle Cerebral Arteries

Though there have been studies on the histopathological and behavioral effects of blast exposure, fewer have been dedicated to blast&#39;s cerebral vascular effects. Impact (i.e., non-blast) traumatic brain injury (TBI) is known to decrease pressure autoregulation in the cerebral vasculature in both humans and experimental animals. The hypothesis that blast-induced traumatic brain injury (bTBI), like impact TBI, results in impaired cerebral vascular reactivity was tested by measuring myogenic dilatory responses to reduced intravascular pressure in rodent middle cerebral arterial (MCA) segments from rats subjected to mild bTBI using an Advanced Blast Simulator (ABS) shock tube. Adult, male Sprague-Dawley rats were anesthetized, intubated, ventilated and prepared for Sham bTBI (identical manipulation and anesthesia except for blast injury) or mild bTBI. Rats were randomly assigned to receive Sham bTBI or mild bTBI followed by sacrifice 30 or 60 min post-injury. Immediately after bTBI, righting reflex (RR) suppression times were assessed, euthanasia at the time points post-injury was completed, the brain was harvested and the individual MCA segments were collected, mounted and pressurized. As the intraluminal pressure perfused through the arterial segments was reduced in 20 mmHg increments from 100 to 20 mmHg, MCA diameters were measured and recorded. With decreasing intraluminal pressure, MCA diameters steadily increased significantly above baseline in the Sham bTBI groups while MCA dilator responses were significantly reduced (p &#60; 0.05) in both bTBI groups as evidenced by the impaired, smaller MCA diameters recorded for the bTBI groups. In addition, RR suppression in the bTBI groups was significantly (p &#60; 0.05) higher than in the Sham bTBI groups. MCA&#39;s collected from the Sham bTBI groups exhibited typical vasodilatory properties to decreases in intraluminal pressure while MCA&#39;s collected following bTBI exhibited significantly impaired myogenic vasodilatory responses to reduced pressure that persisted for at least 60 min after bTBI.

Here, we present a protocol to describe methods for ex vivo vascular reactivity determination following a primary blast traumatic brain injury (bTBI) using isolated, pressurized, rodent middle cerebral arterial (MCA) segments. bTBI induction is accomplished using a shock tube, also known as an Advanced Blast Simulator (ABS) device.

Though there have been studies on the histopathological and behavioral effects of blast exposure, fewer have been dedicated to blast&#39;s cerebral ...

Facial Nerve Surgery in the Rat Model to Study Axonal Inhibition and Regeneration

This protocol describes consistent and reproducible methods to study axonal regeneration and inhibition in a rat facial nerve injury model. The facial nerve can be manipulated along its entire length, from its intracranial segment to its extratemporal course. There are three primary types of nerve injury used for the experimental study of regenerative properties: nerve crush, transection, and nerve gap. The range of possible interventions is vast, including surgical manipulation of the nerve, delivery of neuroactive reagents or cells, and either central or end-organ manipulations. Advantages of this model for studying nerve regeneration include simplicity, reproducibility, interspecies consistency, reliable survival rates of the rat, and an increased anatomic size relative to murine models. Its limitations involve a more limited genetic manipulation versus the mouse model and the superlative regenerative capability of the rat, such that the facial nerve scientist must carefully assess time points for recovery and whether to translate results to higher animals and human studies. The rat model for facial nerve injury allows for functional, electrophysiological, and histomorphometric parameters for the interpretation and comparison of nerve regeneration. It thereby boasts tremendous potential toward furthering the understanding and treatment of the devastating consequences of facial nerve injury in human patients.

This protocol describes a reproducible approach to facial nerve surgery in the rat model, including descriptions of various inducible patterns of injury.

This protocol describes consistent and reproducible methods to study axonal regeneration and inhibition in a rat facial nerve injury model. The facial ...

Using Zebrafish Larvae to Study the Pathological Consequences of Hemorrhagic Stroke

Despite being the most severe subtype of stroke with high global mortality, there is no specific treatment for patients with intracerebral hemorrhage (ICH). Modelling ICH pre-clinically has proven difficult, and current rodent models poorly recapitulate the spontaneous nature of human ICH. Therefore, there is an urgent requirement for alternative pre-clinical methodologies for study of disease mechanisms in ICH and for potential drug discovery.
The use of zebrafish represents an increasingly popular approach for translational research, primarily due to a number of advantages they possess over mammalian models of disease, including prolific reproduction rates and larval transparency allowing for live imaging. Other groups have established that zebrafish larvae can exhibit spontaneous ICH following genetic or chemical disruption of cerebrovascular development. The aim of this methodology is to utilize such models to study the pathological consequences of brain hemorrhage, in the context of pre-clinical ICH research. By using live imaging and motility assays, brain damage, neuroinflammation and locomotor function following ICH can be assessed and quantified.
This study shows that key pathological consequences of brain hemorrhage in humans are conserved in zebrafish larvae highlighting the model organism as a valuable in vivo&#160;system for pre-clinical investigation of ICH. The aim of this methodology is to enable the pre-clinical stroke community to employ the zebrafish larval model as an alternative complementary model system to rodents.

Here we present a protocol to quantify brain injury, locomotor deficits and neuroinflammation following bleeding in the brain in zebrafish larvae, in the context of human intracerebral hemorrhage (ICH).

Despite being the most severe subtype of stroke with high global mortality, there is no specific treatment for patients with intracerebral hemorrhage ...

Combining Behavior and EEG to Study the Effects of Mindfulness Meditation on Episodic Memory

Although there has been recent interest in how mindfulness meditation can affect episodic memory as well as brain structure and function, no study has examined the behavioral and neural effects of mindfulness meditation on episodic memory. Here we present a protocol that combines mindfulness meditation training, an episodic memory task, and EEG to examine how mindfulness meditation changes behavioral performance and the neural correlates of episodic memory. Subjects in a mindfulness meditation experimental group were compared to a waitlist control group. Subjects in the mindfulness meditation experimental group spent four weeks training and practicing mindfulness meditation. Mindfulness was measured before and after training using the Five Facet Mindfulness Questionnaire (FFMQ). Episodic memory was measured before and after training using a source recognition task. During the retrieval phase of the source recognition task, EEG was recorded. The results showed that mindfulness, source recognition behavioral performance, and EEG theta power in right frontal and left parietal channels increased following mindfulness meditation training. In addition, increases in mindfulness correlated with increases in theta power in right frontal channels. Therefore, results obtained from combining mindfulness meditation training, an episodic memory task, and EEG reveal the behavioral and neural effects of mindfulness meditation on episodic memory.

Here we present a protocol for combining mindfulness meditation training, an episodic memory task, and EEG to understand the behavioral and neural effects of mindfulness meditation on episodic memory.

Although there has been recent interest in how mindfulness meditation can affect episodic memory as well as brain structure and function, no study has ...

A Scalable Model to Study the Effects of Blunt-Force Injury in Adult Zebrafish

Podsumowanie

Przeglądaj więcej filmów

Rozdziały w tym wideo

An Optic Nerve Crush Injury Murine Model to Study Retinal Ganglion Cell Survival

Micromanipulation of Gene Expression in the Adult Zebrafish Brain Using Cerebroventricular Microinjection of Morpholino Oligonucleotides

Electrophysiological Recording in the Brain of Intact Adult Zebrafish

Stab Wound Injury of the Zebrafish Adult Telencephalon: A Method to Investigate Vertebrate Brain Neurogenesis and Regeneration

The Olfactory System as a Model to Study Axonal Growth Patterns and Morphology In Vivo

A Simple One-step Dissection Protocol for Whole-mount Preparation of Adult Drosophila Brains

Effects of Blast-induced Neurotrauma on Pressurized Rodent Middle Cerebral Arteries

Facial Nerve Surgery in the Rat Model to Study Axonal Inhibition and Regeneration

Using Zebrafish Larvae to Study the Pathological Consequences of Hemorrhagic Stroke

Combining Behavior and EEG to Study the Effects of Mindfulness Meditation on Episodic Memory