Development of the model was funded Bill and Melinda Gates Foundation, as well as by NIH grant 5R21NS093154-02 (NICHD).

Procedures were performed in accordance with the NIH Guide for the Care and Use of Laboratory Animals and as part of an approved protocol by the University of Washington Institutional Animal Care and Use Committee.
1. Preparation and LPS Administration
NOTE: Refer to Figure 1 for a timeline of the procedures.
<ol>
	<li>Prior to commencing the procedure, seal, sterilize and autoclave all surgical instruments and surgical drapes. Prepare pre-operative medications in sterile vials. Calculate the flow rate required to replace the air in the hypoxia/hyperoxia chamber with the experimental gas in 8&#8211;10 min.</li>
	<li>Prepare the lipopolysaccharide (LPS from E. coli 055:B5) in sterile saline to produce a concentration of 1 mg/mL. Remove P17 ferret kits from their jills. Weigh and number them. Randomize animals by litter and sex to the control or injured (or treatment) groups.</li>
	<li>Using a 300 &#181;L insulin syringe, administer 3 mg/kg of LPS intraperitoneally to kits in the injury group, and an equivalent volume of sterile saline vehicle (3 &#181;L/g) to control animals.</li>
	<li>Place animals in a chamber within a water bath at 37&#8211;40 &#176;C in order to maintain a target rectal temperature of 36&#8211;37 &#176;C throughout the surgical procedures.</li>
</ol>
2. Anesthesia
<ol>
	<li>During the procedure, continually monitor temperature, respiration rate, and heart rate of the animal.</li>
	<li>Administer buprenorphine (0.05 mg/kg) subcutaneously 30 min before the surgical procedure. Induce anesthesia in a mixture of 3% isoflurane balanced with 100% oxygen. Remove the kit from the induction chamber and place it supine on a draped surgical water blanket set to 37 &#176;C. Transfer anesthesia to the nose cone and reduce isoflurane level to 2&#8211;3%.</li>
</ol>
3. Surgical Preparation
<ol>
	<li>Using small animal clippers remove all hair on the ventral neck region. Shave in a rectangular pattern with care to avoid nicking the skin or generating razor rash. Administer local anesthesia to the shaved area using intradermal lidocaine (4 mg/kg) and bupivacaine (2.5 mg/kg).</li>
	<li>Prepare the neck by alternating application of povidone-iodine and 70% ethanol scrub with sterile cotton swabs. Repeat the scrub such that povidone-iodine and 70% ethanol are each applied 3x in alternating fashion.</li>
	<li>Confirm depth of anesthesia via absence of toe-pinch reflex. Maintain level of isoflurane at the minimum percentage required for a surgical plane of anesthesia. Using sterile disposable cut-out drapes that expose the neck region, drape the animal.</li>
</ol>
4. Bilateral Carotid Artery Ligation
<ol>
	<li>With a single-use #11 scalpel blade, make a 1.5 cm midline incision in the center of the neck. Using fine hemostats and curved forceps, bluntly dissect down to the left carotid artery. Dissect the artery away from the associated neurovascular bundle.</li>
	<li>Using a pair of curved fine forceps, pass a looped 10 cm length of sterile 5-0 silk suture under the artery. Cut the suture in half. Ligate the artery by securely tying both lengths of suture, leaving at least 2 mm between the knots. Transect the left carotid artery between the sutures, taking care to leave the nerve intact.</li>
	<li>Repeat the dissection on the right side. Reversibly ligate the right carotid artery with a single sterile 1/8 inch umbilical tie. Close the wound with surgical skin clips.</li>
	<li>Allow the animal to recover in a temperature-controlled water bath for at least 30 min before hypoxia. 
	NOTE: If the arteries are not fully isolated from the rest of the neurovascular bundle, increased mortality may be seen before or during later hypoxia.</li>
</ol>
5. Sequential Hypoxia, Hyperoxia, and Hypoxia
<ol>
	<li>During hypoxia and hyperoxia, alter water bath temperature as necessary to maintain rectal temperature during hypoxia at 37 &#176;C in the sentinel animal(s).</li>
	<li>Place animals in the injury group in an airtight chamber within a water bath. Continuously monitor oxygen concentration within the chamber, as well as rectal temperature in at least one sentinel animal. Flush the chamber with humidified 9% oxygen (91% nitrogen) then maintain a flow rate of 3&#8211;5 L/min, depending on chamber size. Once the concentration of oxygen in the chamber has reached 9%, continue for 30 min.</li>
	<li>After 30 min, switch gas supply to 80% humidified oxygen (20% nitrogen), and allow the chamber to reach the target concentration based on flow rate and chamber size. Continue for 30 min of hyperoxia. Open the chamber to allow it to more rapidly reach normoxia by equilibrating with room air.</li>
	<li>Seal the chamber, and flush with 9% humidified oxygen. Continuously monitor all animals visually, taking note of animals that display bradypnea. Once the concentration of oxygen in the chamber has reached 9%, continue for 30 min. If intra-hypoxic mortality (respiratory arrest) in any of the animals is seen before the end of the 30 min period, terminate hypoxia immediately.</li>
</ol>
6. Reversal of Right Carotid Artery Ligation
<ol>
	<li>Return animals to the surgical area, and induce anesthesia in a mixture of 3% isoflurane balanced with 100% oxygen. Transfer anesthesia to nose cone and reduce isoflurane level to 2&#8211;3%. Remove the surgical wound clips and re-prepare the wound area with povidone-iodine. Confirm depth of anesthesia via absence of toe-pinch reflex. Maintain the level of isoflurane at the minimum percentage required for a surgical plane of anesthesia. Using sterile disposable cut-out drapes that expose the neck region, drape the animal.</li>
	<li>Using curved forceps, identify and untie the umbilical tape from the right carotid artery. Close the wound with surgical skin clips.</li>
</ol>
7. Recovery and Temperature Management
<ol>
	<li>Return all kits to their jills for 60 min, for nursing and recovery. After 60 min, return injured animals to the water baths at 37&#8211;40 &#176;C for 6 h, adjusting water temperature as needed in order to maintain rectal temperature at 36&#8211;37 &#176;C. Return kits to their jills.</li>
	<li>Remove surgical clips 10&#8211;14 days after surgery (P27&#8211;P31).</li>
</ol>
8. Reflex Testing
<ol>
	<li>Perform all the reflex tests daily from P21&#8211;P28, and at least 3x per week from P28&#8211;P42, whilst remaining blinded to exposure (or treatment) group. Prior to reflex testing, place kits in a chamber with heat assistance (37 &#176;C water bath, heat pad, etc.) for 1 h. For each test, complete all trials per kit before testing the next kit.</li>
	<li>Negative geotaxis (25&#176;)
	<ol>
		<li>Place a flat board (16 &#189; in. x 12 in.) wrapped in an absorbent benchtop protector against an object so that the board forms a 25&#176; angle with the table. Place a kit on the board prone and facing downhill, approximately 75% of the way up the board.</li>
		<li>Ensure the kit&#8217;s body is straight and that it has all four paws gripped against the board before releasing it. As soon as the kit is placed, start the time assessment.</li>
		<li>Record the time when the kit manages to rotate its body 90&#176; relative to its starting position. Record the time at which the kit rotates its body 180&#176; and takes a full step towards the top of the board. Perform 3 trials at the 25&#176; incline before moving onto the next test.</li>
	</ol>
	</li>
	<li>Negative geotaxis (45&#176;)
	<ol>
		<li>Perform 3 trials of the previously described negative geotaxis test again, this time with the board set to a 45&#176; angle.</li>
	</ol>
	</li>
	<li>Cliff aversion
	<ol>
		<li>Place a padded platform around 1 foot below the ledge to minimize injury to kits if they fall.</li>
		<li>Place a kit facing, and perpendicular to, the edge of the lab bench. Ensure the kit&#39;s body is straight, with its front paws flush with the edge. Begin time assessment from the moment the kit is placed. Take care to differentiate between conscious movement away from the cliff and other spontaneous movements that do not involve coordinated walking.</li>
		<li>Record the time when the kit moves its body away from the edge (defined as the kit backing up, turning its body, or moving its front limbs away from the edge). Record the time the kit completes its first step in the opposite direction of the edge (defined as any direction or angle past a 90&#176; rotation from its starting position facing the edge).</li>
		<li>Perform 3 cliff aversion trials per kit before moving onto the next test.</li>
	</ol>
	</li>
	<li>Righting reflex
	<ol>
		<li>Place a kit supine on the bench, holding it gently in that position before releasing it and simultaneously beginning the stopwatch. Record the time that the kit brings itself to rest with all four paws simultaneously flat against the bench in weight-bearing positions. Record the time when the kit takes a full step in any direction (defined as the placement of all four paws to achieve progress in a given direction with no spinning or dragging of the body).</li>
		<li>Perform 5 trials of the righting reflex test per animal.</li>
		<li>After every kit has completed the 5 righting reflex trials, return the litter to the jill.</li>
	</ol>
	</li>
</ol>
9. Catwalk Testing
<ol>
	<li>On P42, remove kits from the jill. Place kits in plastic cages approximately 10 min before testing, so they can acclimate to the environment. Turn the lights off in the testing room to ensure ambient light does not affect catwalk function.</li>
	<li>Create a new experiment in the relevant software. Adjust experimental settings so that the maximum run duration does not exceed 10.00 s and the minimum run duration is not less than 1.50 s. Set the maximum speed variation so it does not exceed 60%. Set a minimum requirement of three compliant runs for each animal.</li>
	<li>Adjust the width of the walkway relative to the size of the animal so that it is able to freely locomote without touching the walls while remaining narrow enough to discourage turning. Add a new detection setting in the Detection settings profiles tab using auto detection. Use the same detection settings for all litters and animals at a given age.</li>
	<li>Thoroughly clean the walkway with a low-lint paper tissue and 70% ethanol before and after each animal. Clean the ferret&#39;s paws regularly to improve accuracy of detection and classification. Once the walkway and animal are prepared, begin trial acquisition.</li>
	<li>Pause acquisition to clean the catwalk if footprints accumulate on the glass, or if animals pass urine or feces. Stop acquisition once the catwalk software has recognized three compliant runs based on the pre-determined experiment settings.</li>
</ol>
10. Open Field Testing (P42)
<ol>
	<li>Use a non-porous acrylic box (55 cm x 55 cm x 40 cm high) painted matte-white. Position the camera so that it is centered directly above box and all four walls are captured. Clean the testing arena with 70% ethanol before first use and between animals.</li>
	<li>In the relevant software, select New From Template and Apply a Pre-defined Template. Continue the set-up procedure by sequentially selecting Subject type: Other; Arena template: Open field, square; Zone template: Center, border, corners; Features to track: Center-point.</li>
	<li>Open Arena Settings and grab the background image from the camera input, making sure that the tops of the arena walls are visible. Calibrate the dimensions of the arena using the scale tool.</li>
	<li>Adjust the pre-defined arena zones by resizing the outlines to fit the wall zones (NW, NE, SW, SE) and floor zones (left top, middle top, right top, left middle, center, right middle, left bottom, middle bottom, right bottom). Validate the set-up to confirm that no zones overlap.</li>
	<li>Open the Acquisition window and press Start Acquisition. Place the ferret at the center of the testing arena oriented in such a way that is consistent for every test subject. Allow the ferret to move freely throughout the arena for a period of 5 min. At the end of the testing period, press Stop Acquisition. Repeat the procedure with the next ferret. 
	NOTE: All experimenters in the room should position themselves to be unobservable by the ferret and remain quiet during the testing period.</li>
</ol>
11. Fixation-perfusion
<ol>
	<li>On P42, deeply anesthetize kits with 5% isoflurane. Administer a pentobarbital overdose (120&#8211;150 mg/kg i.p.). Ensure deep anesthesia by lack of response to toe pinch and loss of respiratory movements.</li>
	<li>Transfer the animal to a fume hood. Open the thorax and clamp the descending aorta using fine hemostats. Cut the right atrium. Using a perfusion pump, perfuse the left ventricle with 60 mL of sterile saline at a rate of 30 mL/min. Perfuse with 60 mL of formalin (10% formaldehyde) at a rate of 30 mL/min.</li>
	<li>Decapitate the carcass, and remove the brain from the skull using scissors, forceps, rongeurs, and a spatula. Take high-resolution photographs of the dorsal, ventral, and lateral aspects of each brain. Post-fix the brain in formalin for at least 48 h.</li>
</ol>
12. Ex Vivo Brain Measurement
<ol>
	<li>Remove the brain from formalin (step 11.3) and place onto a paper towel to absorb excess liquid.</li>
	<li>Using an electronic caliper, measure the height of the brain by placing the tips of the caliper at the dorsal and ventral aspects of the brain. Measure the length of the brain by placing the tips of the caliper at the olfactory bulb and the most posterior border of the occipital lobe. Measure the width of the brain by placing the tips of the caliper at the most lateral portions of the temporal lobes. Weigh the brain.</li>
	<li>Measure the longitudinal fissure (anterior and posterior to the cruciate sulcus), lateral sulci, suprasylvian sulci, coronal sulci, pseudosylvian sulci, ansinate sulci, cruciate sulci, presylvian sulci, lateral gyri, suprasylvian gyri, sigmoid gyri (anterior and posterior), coronal gyri, ectosylvian gyri (anterior and posterior), and orbital gyri. Measure all sulci from the beginning and end of the most distinct portion of the corresponding sulcus. Measure all gyri from the widest aspect of each corresponding gyrus.</li>
	<li>Measure the amount of cerebellum exposed by placing one tip of the caliper at the most posterior point of the longitudinal fissure and placing the other tip of the caliper at the most posterior part of the cerebellum. 
	NOTE: The ferret brain atlas, as found in Biology and Diseases of the Ferret14, was used to develop the ex vivo ferret brain measurements.</li>
</ol>
13. Gross Injury Scoring
<ol>
	<li>Using the photographs taken in step 11.3., apply the scoring criteria in steps 13.2&#8211;13.4 to assess gross brain injury (0&#8211;9 scale) whilst remaining blinded to exposure (or treatment) groups.</li>
	<li>Assess the longitudinal fissure. If it appears normal, assign a score of 0. If it is mildly widened (approximately 2x normal width), but the increase in width is incomplete along length of fissure, assign a score of 1. If it is moderately widened (approximately 2&#8211;3x normal), assign a score of 2. If it is markedly widened, with a visible gap &#62;3x normal width along most of the length of fissure, apply a score of 3.</li>
	<li>Assess the lateral sulci. If they show normal definition, with separation of the lateral gyri and suprasylvian gyri, assign a score of 0. If mild unilateral or bilateral reduced definition of sulcus is seen, particularly in the caudal portion, with minimal narrowing of frontal and temporal lobes relative to the occipital lobes, assign a score of 1.
	<ol>
		<li>If moderately reduced definition of the sulci is seen, with depression of the suprasylvian gyri, narrowing of the coronal and ectosylvian gyri, and mild narrowing of frontal and temporal lobes relative to occipital lobes, assign a score of 2. If unilateral cystic degeneration is seen, with minimal change of the contralateral hemisphere, assign a score of 3. If poor definition of the lateral sulci is present, with bilateral cystic or severe degeneration of the occipital and temporal lobes, assign a score of 4.</li>
	</ol>
	</li>
	<li>Assess the visible portion of the cerebellum. If it appears normal, with (&#60;75% of the vermis and &#60;66% of the hemispheres visible, assign a score of 0. If 75&#8211;90% of the vermis and &#8805;66% of the hemispheres are visible, assign a score of 1. If most of the cerebellum is visible, showing all of the vermis and &#8805;66% of hemispheres, assign a score of 2.</li>
</ol>
14. Data Analysis
<ol>
	<li>For reflex testing data, assign failures a score of 61 s to allow them to be compared to successes at the end of time (60 s), but with a worse ranking in the statistical analysis. Calculate an area under the curve for each animal over time in each of the reflex tests.</li>
	<li>Adjust catwalk data that involves paw size of pressure by the weight of the animal.</li>
	<li>Analyze data using non-parametric statistical methods, describing data using the median and interquartile range (IQR).</li>
</ol>

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The authors have nothing to disclose.

Due to the physical and developmental similarities shared between the ferret brain and human brain, the ferret is increasingly being used to model both adult and developmental brain injury.8,9,10,11,12. However, research to date suggests that the ferret brain is both resistant to initial injury as well as highly-plastic, with behavioral deficits diminishing ov...

There is an ongoing need for large animal models that reflect the pathophysiology of prematurity and perinatal hypoxia-ischemia in which therapeutic interventions for infants can be tested. In 2017, 9.93% of the 382,726 infants born in the United States were born preterm, and 84% of these infants were born between 32 and 36 weeks of gestation1. In premature infants, perinatal exposure to infection or inflammation is common, where maternal immune activation due to viral or bacterial pathogens can initiate preterm labor. Postnatally, preterm infants are at high risk of early or late onset sepsis2. Preterm infants also frequently experience periods of hypoxia, hypotension, and hyperoxia due to their immature cardiorespiratory system, elevated oxygen tension in the atmosphere relative to those experienced in utero, and iatrogenic exposures. Additionally, in preterm infants, antioxidant defenses are immature3 and pro-apoptotic factors are naturally upregulated4. Oxidative stress and cell death lead to activation of the immune system and neuroinflammation. These combined factors are thought to contribute to developmental and physiologic vulnerability of the brain, and result in or exacerbate the encephalopathy associated with poor developmental outcomes in preterm infants5,6,7.
Due to the physical and developmental similarities that the ferret brain shares with the human brain, the ferret is an attractive species in which to model brain injury8,9,10,11,12. Ferrets are also ideal candidates to model the preterm human brain, as they are born lissencephalic and develop gyrencephalic brains postnatally, which provides a window in which to expose the developing brain to insults that mimic those experienced by infants born preterm. At birth, ferret brain development is similar to a 13 week human fetus, with postnatal-day (P) 17 kits considered to be equivalent to an infant at 32&#8211;36 weeks of gestation13.
Our group has recently published a model of extremely preterm (&#60;28 weeks&#39; gestation) brain injury in the P10 ferret by combining inflammatory sensitization with Escherichia coli lipopolysaccharide (LPS) with subsequent exposure to hypoxia and hyperoxia12. In the following protocol, we now describe a late preterm model in the P17 ferret, where LPS sensitization is followed by bilateral cerebral ischemia, hypoxia, and hyperoxia. This results in more severe injury in a subset of animals, and more closely models the complex interaction of prolonged inflammation, ischemia, hypoxia, and oxidative stress experienced in a number of preterm infants who develop brain injury.

<table><tbody><tr><td>80% Oxygen</td><td>Praxair</td><td></td><td></td></tr><tr><td>9% Oxygen</td><td>Praxair</td><td></td><td></td></tr><tr><td>Absorbent benchtop protector</td><td>Kimtech</td><td>7546</td><td></td></tr><tr><td>Automated catwalk</td><td>Noldus</td><td></td><td></td></tr><tr><td>Betadine surgical scrub</td><td></td><td></td><td></td></tr><tr><td>Bupivacaine</td><td>Patterson Veterinary</td><td>07-888-9382</td><td></td></tr><tr><td>Buprenorphine</td><td></td><td></td><td></td></tr><tr><td>Calipers</td><td>SRA Measurement Products</td><td>ME-CAL-FP-200</td><td>200 mm range, 0.01 mm resolution</td></tr><tr><td>Cotton Gauze Sponge</td><td>Fisher Scientific</td><td>22028556</td><td></td></tr><tr><td>Curved fine hemostat</td><td>Roboz</td><td>RS-7101</td><td></td></tr><tr><td>Curved forceps</td><td>World Precision Instruments</td><td>501215</td><td></td></tr><tr><td>Curved suture-tying hemostat</td><td>Roboz</td><td>RS-7111</td><td></td></tr><tr><td>Ethovision tracking software</td><td>Noldus</td><td></td><td></td></tr><tr><td>Eye Lubricant</td><td>Rugby</td><td>NDC 0536-1970-72</td><td></td></tr><tr><td>Ferrets (Mustela putorius furo)</td><td>Marshall Biosciences</td><td></td><td>Outbred (no specific strain)</td></tr><tr><td>Formalin</td><td>Fisher Scientific</td><td>SF100-4</td><td>10% (Phosphate Buffer/Certified)</td></tr><tr><td>Hair Clippers</td><td>Conair</td><td>GMT175N</td><td></td></tr><tr><td>Insulin Syringes</td><td>BD</td><td>329461</td><td>0.3 cc 3 mm 31 G</td></tr><tr><td>Isoflurane</td><td>Piramal</td><td>66794-017-25</td><td></td></tr><tr><td>Lidocaine</td><td>Patterson Veterinary</td><td>07-808-8202</td><td></td></tr><tr><td>LPS</td><td>List Biological</td><td>LPS Ultrapure #423</td><td></td></tr><tr><td>Oxygen sensor</td><td>BW Gas Alert</td><td>GAXT-X-DL-2</td><td></td></tr><tr><td>Pentobarbital</td><td></td><td></td><td></td></tr><tr><td>Plastic chamber</td><td>Tellfresh</td><td>1960</td><td>10 L; 373 x 270 x 135 mm&lt;sup&gt;3&lt;/sup&gt;</td></tr><tr><td>Saline Solution, 0.9%</td><td>Hospira</td><td>RL-4492</td><td></td></tr><tr><td>Scalpel blade</td><td>Integra Miltex</td><td>297</td><td></td></tr><tr><td>Scalpel handle</td><td>World Precision Instruments</td><td>500236</td><td>#3, 13 cm</td></tr><tr><td>Sterile suture</td><td>Fine Science Tools</td><td>18020-50</td><td>Braided Silk, 5/0</td></tr><tr><td>Surgical clip applicator</td><td>Fine Science Tools</td><td>12020-09</td><td></td></tr><tr><td>Surgical clip remover</td><td>Fine Science Tools</td><td>12023-00</td><td></td></tr><tr><td>Surgical drapes</td><td>Medline Unidrape</td><td>VET3000</td><td></td></tr><tr><td>Surgical gloves</td><td>Ansell Perry Inc</td><td>5785004</td><td></td></tr><tr><td>Surigical clips</td><td>Fine Science Tools</td><td>12022-09</td><td></td></tr><tr><td>Thermometer (rectal)</td><td>YSI</td><td>Precision 4000A</td><td></td></tr><tr><td>Thermometer (water)</td><td>Fisher Scientific</td><td>14-648-26</td><td></td></tr><tr><td>Umbilical tape</td><td>Grafco</td><td>3031</td><td>Sterile</td></tr><tr><td>Water bath</td><td>Thermo Scientific</td><td>TSCOL19</td><td>19 L</td></tr></tbody></table>

a ferret model of inflammation-sensitized late preterm hypoxic-ischemic brain injury

There is an ongoing need for clinically relevant models of perinatal infection and hypoxia-ischemia (HI) in which to test therapeutic interventions for infants with the neurological sequela of prematurity. Ferrets are ideal candidates for modeling the preterm human brain, as they are born lissencephalic and develop gyrencephalic brains postnatally. At birth, ferret brain development is similar to a 13 week human fetus, with postnatal-day (P) 17 kits considered to be equivalent to an infant at 32&#8211;36 weeks&#39; gestation. We describe an injury model in the P17 ferret, where lipopolysaccharide administration is followed by bilateral cerebral ischemia, hypoxia, and hyperoxia. This simulates the complex interaction of prolonged inflammation, ischemia, hypoxia, and oxidative stress experienced in a number of neonates who develop brain injury. Injured animals display a range of gross injury severity, with morphological changes in the brain including narrowing of multiple cortical gyri and associated sulci. Injured animals also show slowed reflex development, slower and more variable speed of locomotion in an automated catwalk, and decreased exploration in an open field. This model provides a platform in which to test putative therapies for infants with neonatal encephalopathy associated with inflammation and HI, study mechanisms of injury that affect cortical development, and investigate pathways that provide resilience in unaffected animals.

Of 34 (n = 18 males, n = 16 females) animals from six litters exposed to the insult, eight animals (24%; n = 4 males, n = 4 females) in the injured group died during the second hypoxia period (n = 5), during temperature management (n = 2), or overnight after the insult (n = 1). In the injured group, nine of 26 survivors (35%) had visible gross injury. Five animals (n = 5 males) had moderate injury, and four animals (n = 2 males, n = 2 females) had severe injury, defined as gross pathology scores of 2&#8211;5 and 6&#8211;...

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A Ferret Model of Inflammation-sensitized Late Preterm Hypoxic-ischemic Brain Injury

The method describes inflammation-sensitized hypoxic-ischemic and hyperoxic brain injury in the P17 ferret to model the complex interaction between prolonged inflammation and oxidative brain injury experienced in a number of late preterm infants.

There is an ongoing need for clinically relevant models of perinatal infection and hypoxia-ischemia (HI) in which to test therapeutic interventions for ...

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Research

JoVE Journal

Neuroscience

7.5K Views.  University of Washington. Dit protocol is belangrijk omdat het biedt het eerste model van ontsteking gesensibiliseerd voortijdig hersenletsel in de fretten die resulteert in aanzienlijke en aanhoudende schade. Deze techniek omvat een langdurige beledigingen die veel van de triggers en biochemische mechanismen dacht bij te dragen aan de soorten hersenletsel gezien bij premature menselijke zuigelingen bevat. Het aantonen van de hersenen meting procedure zal Kylie Corry, een onderzoeker in ons lab en Olivia White, een st...

Video: A Ferret Model of Inflammation-sensitized Late Preterm Hypoxic-ischemic Brain Injury

Mouse Models of Periventricular Leukomalacia

We describe a protocol for establishing mouse models of periventricular leukomalacia (PVL). PVL is the predominant form of brain injury in premature infants and the most common antecedent of cerebral palsy. PVL is characterized by periventricular white matter damage with prominent oligodendroglial injury. Hypoxia/ischemia with or without systemic infection/inflammation are the primary causes of PVL. We use P6 mice to create models of neonatal brain injury by the induction of hypoxia/ischemia with or without systemic infection/inflammation with unilateral carotid ligation followed by exposure to hypoxia with or without injection of the endotoxin lipopolysaccharide (LPS). Immunohistochemistry of myelin basic protein (MBP) or O1 and electron microscopic examination show prominent myelin loss in cerebral white matter with additional damage to the hippocampus and thalamus. Establishment of mouse models of PVL will greatly facilitate the study of disease pathogenesis using available transgenic mouse strains, conduction of drug trials in a relatively high throughput manner to identify candidate therapeutic agents, and testing of stem cell transplantation using immunodeficiency mouse strains.

We established mouse models of periventricular leukomalacia (PVL), the predominant brain injury in premature infants characterized by periventricular white matter lesions. Hypoxia/ischemia with/without systemic infection are the primary causes of PVL. Unilateral carotid ligation and hypoxia exposure with/without lipopolysaccharide injection creates PVL-like lesions in P6 mice.

We describe a protocol for establishing mouse models of periventricular leukomalacia (PVL). PVL is the predominant form of brain injury in premature ...

The Hypoxic Ischemic Encephalopathy Model of Perinatal Ischemia

Hypoxic-Ischemic Encephalopathy (HIE) is the consequence of systemic asphyxia occurring at birth. Twenty five percent of neonates with HIE develop severe and permanent neuropsychological sequelae, including mental retardation, cerebral palsy, and epilepsy. The outcomes of HIE are devastating and permanent, making it critical to identify and develop therapeutic strategies to reduce brain injury in newborns with HIE. To that end, the neonatal rat model for hypoxic-ischemic brain injury has been developed to model this human condition. The HIE model was first validated by Vannucci et al 1 and has since been extensively used to identify mechanisms of brain injury resulting from perinatal hypoxia-ischemia 2 and to test potential therapeutic interventions 3,4. The HIE model is a two step process and involves the ligation of the left common carotid artery followed by exposure to a hypoxic environment. Cerebral blood flow (CBF) in the hemisphere ipsilateral to the ligated carotid artery does not decrease because of the collateral blood flow via the circle of Willis; however with lower oxygen tension, the CBF in the ipsilateral hemisphere decreases significantly and results in unilateral ischemic injury. The use of 2,3,5-triphenyltetrazolium chloride (TTC) to stain and identify ischemic brain tissue was originally developed for adult models of rodent cerebral ischemia 5, and is used to evaluate the extent of cerebral infarctin at early time points up to 72 hours after the ischemic event 6. In this video, we demonstrate the hypoxic-ischemic injury model in postnatal rat brain and the evaluation of the infarct size using TTC staining.

The postnatal rat model for hypoxic-ischemic brain injury is a well-established model of human neonatal hypoxic ischemic encephalopathy (HIE). In this article, we describe the model of HIE in post-natal rat pups.

Hypoxic-Ischemic Encephalopathy (HIE) is the consequence of systemic asphyxia occurring at birth. Twenty five percent of neonates with HIE develop severe ...

Biology

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

Modeling Encephalopathy of Prematurity Using Prenatal Hypoxia-ischemia with Intra-amniotic Lipopolysaccharide in Rats

Encephalopathy of prematurity (EoP) is a term that encompasses the central nervous system (CNS) abnormalities associated with preterm birth. To best advance translational objectives and uncover new therapeutic strategies for brain injury associated with preterm birth, preclinical models of EoP must include similar mechanisms of prenatal global injury observed in humans and involve multiple components of the maternal-placental-fetal system. Ideally, models should produce a similar spectrum of functional deficits in the mature animal and recapitulate multiple aspects of the pathophysiology. To mimic human systemic placental perfusion defects, placental underperfusion and/or chorioamnionitis associated with pathogen-induced inflammation in early preterm birth, we developed a model of prenatal transient systemic hypoxia-ischemia (TSHI) combined with intra-amniotic lipopolysaccharide (LPS). In pregnant Sprague Dawley rats, TSHI via uterine artery occlusion on embryonic day 18 (E18) induces a graded placental underperfusion defect associated with increasing CNS damage in the fetus. When combined with intra-amniotic LPS injections, placental inflammation is increased and CNS damage is compounded with associated white matter, gait and imaging abnormalities. Prenatal TSHI and TSHI+LPS prenatal insults meet several of the criteria of an EoP model including recapitulating the intrauterine insult, causing loss of neurons, oligodendrocytes and axons, loss of subplate, and functional deficits in adult animals that mimic those observed in children born extremely preterm. Moreover, this model allows for the dissection of inflammation induced by divergent injury types.

Encephalopathy of prematurity encompasses the central nervous system abnormalities associated with injury from preterm birth. This report describes a clinically relevant rat model of in utero transient systemic hypoxia-ischemia and intra-amniotic lipopolysaccharide administration (LPS) that mimics chorioamnionitis, and the related impact of infectious stimuli and placental underperfusion on CNS development.

Encephalopathy of prematurity (EoP) is a term that encompasses the central nervous system (CNS) abnormalities associated with preterm birth. To best ...

Neurobehavioral Assessments in a Mouse Model of Neonatal Hypoxic-ischemic Brain Injury

We performed unilateral carotid artery occlusion on CD-1 mice to create a neonatal hypoxic-ischemic (HI) model and investigated the effects of neonatal HI brain injury by studying neurobehavioral functions in these mice compared to non-operated (i.e., normal) mice. During the study, Rice-Vannucci&#39;s method was used to induce neonatal HI brain damage in postnatal day 7-10 (P7-10) mice. The HI operation was performed on the pups by unilateral carotid artery ligation and exposure to hypoxia (8% O2 and 92% N2 for 90 min). One week after the operation, the damaged brains were evaluated with the naked eye through the semi-transparent skull and were categorized into subgroups based on the absence (&#34;no cortical injury&#34; group) or presence (&#34;cortical injury&#34; group) of cortical injury, such as a lesion in the right hemisphere. On week 6, the following neurobehavioral tests were performed to evaluate the cognitive and motor functions: passive avoidance task (PAT), ladder walking test, and grip strength test. These behavioral tests are helpful in determining the effects of neonatal HI brain injury and are used in other mouse models of neurodegenerative diseases. In this study, neonatal HI brain injury mice showed motor deficits that corresponded to right hemisphere damage. The behavioral test results are relevant to the deficits observed in human neonatal HI patients, such as cerebral palsy or neonatal stroke patients. In this study, a mouse model of neonatal HI brain injury was established and showed different degrees of motor deficits and cognitive impairment compared to non-operated mice. This work provides basic information on the HI mouse model. MRI images demonstrate the different phenotypes, separated according to the severity of brain damage by motor and cognitive tests.

We performed unilateral carotid artery occlusion on postnatal day 7-10 CD-1 mouse pups to create a neonatal hypoxic-ischemic (HI) model and investigated the effects of HI brain injury. We studied neurobehavioral functions in these mice compared to non-operated normal mice.

We performed unilateral carotid artery occlusion on CD-1 mice to create a neonatal hypoxic-ischemic (HI) model and investigated the effects of neonatal HI ...

Transient Middle Cerebral Artery Occlusion Model of Neonatal Stroke in P10 Rats

A number of animal models have been used to study hypoxic-ischemic injury, traumatic injury, global hypoxia, or permanent ischemia in both the immature and mature brain. Stroke occurs commonly in the perinatal period in humans, and transient ischemia-reperfusion is the most common form of stroke in neonates. The reperfusion phase is a critical component of injury progression, which occurs over a period of days to weeks, and of the endogenous response to injury. This postnatal day 10 (p10) rat model of transient middle cerebral artery occlusion (tMCAO) creates a unilateral, non-hemorrhagic focal ischemia-reperfusion injury that can be utilized to study the mechanisms of focal injury and repair in the full-term-equivalent brain. The injury pattern that is produced by tMCAO is consistent and highly reproducible and can be confirmed with MRI or histological analyses. The severity of injury can be manipulated through changes in occlusion time and other methods that will be discussed.

Neonatal stroke is a significant cause of early brain injury requiring a translational model with consistent focal injury patterns and high reproducibility in order to enable study. This study describes the detailed surgical procedure for creating a non-hemorrhagic, unilateral focal ischemia-reperfusion injury in full-term-equivalent rodents.

A number of animal models have been used to study hypoxic-ischemic injury, traumatic injury, global hypoxia, or permanent ischemia in both the immature ...

A Preclinical Controlled Cortical Impact Model for Traumatic Hemorrhage Contusion and Neuroinflammation

Cerebral contusion is a severe medical problem affecting millions of people worldwide each year. There is an urgent need to understand the pathophysiological mechanism and to develop effective therapeutic strategy for this devastating neurological disorder. Intraparenchymal hemorrhage and post-traumatic inflammatory response induced by initial physical impact can aggravate microglia/macrophage activation and neuroinflammation which subsequently worsen brain pathology. We provide here a controlled cortical impact (CCI) protocol that can reproduce experimental cortical contusion in mice by using a pneumatic impactor system to deliver mechanical force with controllable magnitude and velocity onto the dural surface. This preclinical model allows researchers to induce moderately severe focal cerebral contusion in mice and to investigate a wide range of post-traumatic pathological progressions including hemorrhage contusion, microglia/macrophage activation, iron toxicity, axonal injury, as well as short-term and long-term neurobehavioral deficits. The present protocol can be useful for exploring the long-term effects of and potential interventions for cerebral contusion.

Intraparenchymal hemorrhage and neuroinflammation accompanied by cerebral contusion can trigger severe secondary brain injury. This protocol details a mouse controlled cortical impact (CCI) model allowing researchers to study hemorrhage contusion and post-traumatic immune responses and explore potential therapeutics.

Cerebral contusion is a severe medical problem affecting millions of people worldwide each year. There is an urgent need to understand the ...

Early Pathological and Magnetic Resonance Detection of Cerebral Injury Using a Rat Model of Neonatal Hypoxic Ischemic Encephalopathy

Perinatal hypoxic-ischemic encephalopathy (HIE) is an acute disease that may afflict newborns, resulting in variable long- and short-term neurodevelopmental outcomes. Early diagnosis is critical to identifying infants who may benefit from intervention; however, early diagnosis relies heavily on clinical criteria. No molecular or radiological tests have shown promise in detecting early cerebral injury. Studies have shown that magnetic resonance imaging (MRI) can show changes in both blood flow/ischemia and metabolic disruption. However, they have all been used to evaluate the secondary phase of the disease (&gt;12 h) after the onset of the injury. Early diagnosis is critical to rapidly starting therapeutic hypothermia in eligible infants, which is currently recommended to be initiated within 6 h of birth. The rat model of hypoxic-ischemic injury was developed in 1981 and has been validated and used extensively to study changes in brain perfusion, cerebral injury markers, and morphology. However, it has primarily been used as a "late model", evaluating injury several days after the initial ischemic insult. The model has been known to have poor sensitivity in evaluating reliable and reproducible early cerebral changes. The objective of this study was to develop a reliable model to study early gross morphological and radiological markers of HIE using pathological staining and cerebral magnetic resonance imaging/magnetic resonance spectroscopy.

The present protocol describes a rodent model of newborn hypoxic-ischemic injury for identifying early changes in cerebral tissue by gross morphology and magnetic resonance imaging. This has benefits over existing models, which can be used to study late injury but do not allow the evaluation of reproducible early changes.

Perinatal hypoxic-ischemic encephalopathy (HIE) is an acute disease that may afflict newborns, resulting in variable long- and short-term ...

Modeling Posthemorrhagic Hydrocephalus of Prematurity in Rats

Posthemorrhagic hydrocephalus of prematurity (PHHP) is a serious sequela of severe intraventricular hemorrhage (IVH) in very preterm infants less than 32 weeks gestational age (GA). PHHP is defined by the accumulation of cerebrospinal fluid (CSF) associated with clinical symptoms of elevated intracranial pressure (ICP). Infants with PHHP suffer lifelong shunt dependence, with half requiring repeat surgery in the first year of life and many requiring multiple additional surgeries throughout the lifespan. Prenatal chorioamnionitis predisposes preterm infants to severe IVH and the need for surgical treatment of PHHP trends with neonatal sepsis. These clinical features suggest that systemic inflammation is an integral component of PHHP pathophysiology. 
Here, we define an animal model that recapitulates all clinical aspects and essential features of PHHP in rats. The goal of this protocol is to illustrate how in utero chorioamnionitis and postnatal IVH using lysed red blood cells can be combined to yield PHHP. This preclinical approach yields progressive macrocephaly and domed craniums, elevated intracranial pressure, and ventriculomegaly that can be detected via magnetic resonance imaging (MRI) or via microscopy. In addition to sustained disruption in CSF dynamics, rats also have cognitive delay and functional disability into adulthood. Accordingly, this preclinical platform facilitates unique and unparalleled translational studies of PHHP that can incorporate molecular, cellular, biochemical, histologic, imaging, and functional outcome measures. It can also be used for rigorous analysis of the choroid plexus, ependymal motile cilia, and glymphatic system in parallel. Last, it can also be an invaluable preclinical tool for the investigation of novel surgical intervention strategies and non-surgical therapeutic approaches for the treatment of hydrocephalus.

Posthemorrhagic hydrocephalus of prematurity (PHHP) can be modeled in neonatal rats by combining chorioamnionitis and intraventricular hemorrhage. The combination of these prenatal and postnatal events accurately recapitulates the clinical hallmarks of PHHP, including macrocephaly, ventriculomegaly, and elevated intracranial pressure, through the lifespan.

Posthemorrhagic hydrocephalus of prematurity (PHHP) is a serious sequela of severe intraventricular hemorrhage (IVH) in very preterm infants less than 32 ...

Establishing a Mouse Model of Neonatal Hypoxic-Ischemic Brain Injury

Source: Kim, M., et al. <a href="https://app.jove.com/v/55838">Neurobehavioral Assessments in a Mouse Model of Neonatal Hypoxic-ischemic Brain Injury.</a> J. Vis. Exp. (2017).
The video demonstrates the procedure for creating a mouse model to study neonatal hypoxic-ischemic brain injury. It outlines the steps for surgically inducing ischemia and subjecting the animal to hypoxia to exacerbate brain damage. Finally, it shows how to assess the resulting brain lesions, ensuring the mouse model is prepared for further scientific investigation.

A Ferret Model of Inflammation-sensitized Late Preterm Hypoxic-ischemic Brain Injury

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