JMS received funding from NIH/NINDS R01 NS110793 and K12 (Neurosurgeon Research Career Development Program). BAM received funding from NIH/NINDS K08 NS112580-01A1, University of Kentucky Neuroscience Research Priority Area Award, and a Hydrocephalus Association Innovator Award.

NOTE: All animal protocols were approved by the institutions&#39; Animal Care and Use Committee. See the Table of Materials for details about all materials, reagents, equipment, and software used in this protocol.
1. Preparation of hemoglobin and CSF solutions
<ol>
	<li>Prepare a sterile&#160;artificial CSF (aCSF) solution by adding 500 &#181;L of the aCSF solution to a 1.5 mL microtube and store on ice.</li>
	<li>Prepare a sterile 150 mg/mL hemoglobin solution by adding 75 mg of hemoglobin to 500 &#181;L of aCSF in a 1.5 mL microtube and store on ice.</li>
</ol>
2. Preparation of the animal for injection
<ol>
	<li>Turn the heating pad to the medium setting to maintain the body temperature of the rat.</li>
	<li>Anesthetize postnatal day 4 (P4) rats in an induction chamber filled with 3% isoflurane. 
	NOTE: Confirm sufficient anesthesia using the toe/tail-pinch response every 15 min. Monitor anesthesia with visual observation of tissue color, body temperature, and respiratory rate.</li>
	<li>Administer pain relief with a 5 mg/kg subcutaneous carprofen injection to the anesthetized rat.</li>
	<li>Place the anesthetized rat prone in the stereotactic apparatus with the nose positioned in the anesthesia adaptor with a constant flow of 1.5% isoflurane.</li>
	<li>Tighten non-rupture ear bars on the external auditory meatus to secure the head. 
	NOTE: Apply vet ointment to keep the eyes moisturized if the eyes are open at the age of injection.</li>
	<li>Clean the head, alternating with sterile cotton-tipped applicators soaked in betadine and 70% ethanol.
	<ol>
		<li>Touch the betadine-soaked applicator to the center of the scalp and spread the betadine in circles, moving outward.</li>
		<li>Repeat step 2.6.1.1 with the ethanol-soaked applicator.</li>
		<li>Repeat step 2.6.1.1 and step 2.6.1.2 3x.</li>
	</ol>
	</li>
	<li>Apply a sterile surgical drape to protect the surgical field.&#160;</li>
	<li>Using a sterile scalpel, make a 0.3 cm incision vertically down the center of the head to expose the bregma of the skull. 
	NOTE: If injecting from the lambda, expose the lambda of the skull instead of the bregma.</li>
	<li>Use a sterile cotton-tipped applicator to dry the area.</li>
</ol>
3. Setting up the stereotactic injector
<ol>
	<li>Draw the hemoglobin solution prepared in step 1.2 into a 0.3 mL sterile syringe with a 30G needle and place the syringe into the stereotactic injector system. 
	&#8203;NOTE: If generating control conditions, draw aCSF solution prepared in step 1.1 into a 0.3 mL sterile syringe and proceed with the protocol.</li>
	<li>Turn on the stereotactic injector interface and click on the Configuration button to input the injection volume and rate settings.
	<ol>
		<li>Click on Volume and set the volume at 20,000 nL (20 &#181;L).</li>
		<li>Click on Infusion rate and set the rate at 8,000 nL/min (8 &#181;L/min).</li>
	</ol>
	</li>
	<li>Exit Configuration by clicking on the Reset Pos&#160;button.</li>
	<li>Flush the needle tip by clicking on the Infuse button until a small bead of hemoglobin solution emerges at the needle tip.</li>
	<li>Gently wick the hemoglobin solution from the needle tip with a sterile cotton-tipped applicator.</li>
</ol>
4. Animal injection
<ol>
	<li>Set the bregma as zero on the stereotactic injector system by adjusting the mediolateral and anteroposterior positions of the syringe before lowering the tip of the flushed syringe needle to gently touch the skull at the bregma. 
	NOTE: If injecting from the lambda, set lambda as zero.</li>
	<li>Identify the coordinates of choice.
	<ol>
		<li>If injecting from the bregma, in P4 rats described here, use 1.5 mm lateral, 0.4 mm anterior, and 2.0 mm deep from bregma.</li>
		<li>If injecting from the lambda, use the following coordinates for P4 rats: 1.1 mm lateral, 4.6 mm anterior, and 3.3 mm deep from lambda.</li>
	</ol>
	</li>
	<li>Raise the syringe needle 1 cm above the skull to clear the scalp. When the syringe is raised, proceed to set the mediolateral and anteroposterior coordinates.</li>
	<li>Lower the syringe needle to gently touch the skull. Check that the needle is touching the skull.</li>
	<li>Set the dorsoventral coordinate over a 30 s period. 
	NOTE: While setting the dorsoventral coordinate, the needle will puncture the skull. Care must be taken to assure that the syringe passes through the skull without deforming the skull. Skull deformation is avoided by slowly withdrawing the needle along the dorsoventral coordinate if deformation occurs, then placing the needle back along the same trajectory. This allows the needle to pass through the hole in the skull with less force and no deformation.</li>
	<li>On the stereotactic injector interface, click on the Run button to begin injection.</li>
	<li>After the injection is finished, leave the syringe needle in place for 2 min to minimize backflow of the solution.</li>
	<li>Withdraw the syringe slowly along the dorsoventral coordinate over 2&#160;min until the needle tip is 2 cm above the scalp.</li>
	<li>Rotate the stereotactic injector arm away from the operative field.</li>
</ol>
5. Postoperative care
<ol>
	<li>Close the scalp with a 6-0 monofilament suture. Make one simple interrupted suture at the center of the 0.3 cm incision.</li>
	<li>Remove the pup from anesthesia and place it onto a secure area on the heating pad.</li>
	<li>Return the rodent to the home cage to recover from the anesthesia under the care of its dam. 
	NOTE: Timely return to the care of the dam reduces early postoperative mortality.</li>
	<li>Monitor the animals for anesthesia by loss of the righting reflex hourly post surgery for 3 h.</li>
	<li>Monitor the animals daily for 7 days for normal activity, food intake, and weight gain. Monitor the incision site for wound healing, closure, and reappearance of fur at the site of surgery. 
	NOTE: In the rare case that neurological changes such as seizures, central depression, or decreased appetite are observed during monitoring, euthanize the animal using intravascular perfusion or cervical dislocation under anesthesia.</li>
	<li>To prevent infection once the suture is closed and the wound is healing, apply topical triple-antibiotic at the incision site.</li>
</ol>
6. MRI acquisition and quantification
<ol>
	<li>Perform MRI on a 4.7T or 9.4T small-animal scanner.</li>
	<li>Turn the heating pad to the medium setting to maintain the body temperature of the rat.</li>
	<li>Induce anesthesia in a chamber using 3% isoflurane. 
	NOTE: Confirm sufficient anesthesia using the toe/tail-pinch response every 15 min. Monitor anesthesia with visual observation of tissue color, body temperature, and respiratory rate.</li>
	<li>Place the anesthetized rat prone in the MRI with the nose positioned in the anesthesia adaptor with a constant flow of 1.5% isoflurane.</li>
	<li>Perform T2-weighted imaging by selecting a T2-weighted fast spin echo sequence.
	<ol>
		<li>If using a 4.7T MRI scanner, enter the following parameters into the MRI software: repetition&#8239;time = 3,000 ms, echo time = 27.50 ms, number of averages = 3, field of view = 18.0 mm x 18.0 mm, matrix = 128 x 128, number of axial slices = 24, thickness = 0.50 mm.</li>
		<li>If using a 9.4T MRI scanner, enter the following parameters into the MRI software: repetition time = 5,000 ms, echo time = 66.00 ms, echo spacing = 16.50 ms, number of averages = 2, repetitions = 1, rare factor = 8, field of view = 16.0 mm x 16.0 mm, matrix = 256 x 256, number of axial slices = 32, thickness = 0.50 mm.</li>
	</ol>
	</li>
	<li>Click on the Continue button to start the sequence.</li>
</ol>
7. Image processing and analysis
<ol>
	<li>Use native T2-weighted data to analyze brain volume. Use segmentation software to manually delineate the lateral ventricles6. Click on Paintbrush Mode and select square brush style. Adjust the brush size to 1. Click Layout inspector and select axial view. Click zoom to fit. Place the cursor on the image; trace and fill the lateral ventricle space.</li>
	<li>Click on Segmentation in the toolbar | Volume and Statistics to view the segmented volumes.</li>
</ol>

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<li>Cherian, S. S., Love, S., Silver, I. A., Porter, H. J., Whitelaw, A. G. L., Thoresen, M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Posthemorrhagic+ventricular+dilation+in+the+neonate%3A+Development+and+characterization+of+a+rat+model%5BTitle%5D)+AND+%22Journal+of+Neuropathology+and+Experimental+Neurology%22%5BJournal%5D)">Posthemorrhagic ventricular dilation in the neonate: Development and characterization of a rat model.</a> Journal of Neuropathology and Experimental Neurology. 62 (3), (2003).</li>
<li>Balasubramaniam, J., Xue, M., Buist, R. J., Ivanco, T. L., Natuik, S., del Bigio,, R, M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Persistent+motor+deficit+following+infusion+of+autologous+blood+into+the+periventricular+region+of+neonatal+rats%5BTitle%5D)+AND+%22Experimental+Neurology%22%5BJournal%5D)">Persistent motor deficit following infusion of autologous blood into the periventricular region of neonatal rats.</a> Experimental Neurology. (1), (2006).</li>
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The authors declare that they have no conflicts of interest.

This IVH model utilizing hemoglobin injection allows for the study of the pathology of IVH specifically mediated by hemoglobin. For complementary studies, hemoglobin can also be easily delivered in vitro and does not confound biochemical assays for proteins made by microglia/macrophages that are present in whole blood.
The leading theories of IVH-PHH include the mechanical obstruction of CSF circulation, the disruption of cilia lining the ependymal walls, inflammation, fibrosis, and i...

Neonatal IVH originates from the germinal matrix, a site of rapid cell division that is adjacent to the lateral ventricles of the developing brain. This highly vascular structure is vulnerable to hemodynamic instability related to premature birth. Blood is released into the lateral ventricles in germinal matrix hemorrhage (GMH)-IVH when fragile blood vessels within the germinal matrix rupture. In the case of grade IV IVH, periventricular hemorrhagic infarction may also contribute to the release of blood products within the brain.1 The combination of GMH-IVH may cause PHH, particularly after high-grade hemorrhage (grades III and IV)1. PHH can be treated with the placement of a ventriculoperitoneal shunt, but shunt placement does not reverse the brain injury that may occur from IVH. Although modern neonatal intensive care has lowered rates of IVH2, 3, there are no specific treatments for the brain injury or hydrocephalus caused by IVH once it has occurred. A significant limitation in developing preventative treatments for IVH-induced brain injury and PHH is the incomplete understanding of IVH pathophysiology.
Recently, early CSF levels of key blood breakdown product hemoglobin have been shown to be associated with the later development of PHH in neonates with high-grade IVH4. Furthermore, CSF levels of iron-handling pathway proteins&#8212;hemoglobin, ferritin, and bilirubin&#8212;are associated with ventricle size in neonatal IVH. This was also shown in a multicenter cohort of infants with preterm PHH, where higher ventricular CSF levels of ferritin were associated with larger ventricle size5.
In this study, we developed a clinically relevant model of IVH-induced brain injury and hydrocephalus utilizing hemoglobin injection into the brain ventricles, which allows for quantification of brain injury and PHH and the testing of new therapeutic strategies (Figure 1)6, 7. This IVH model utilizes neonatal rat pups, which are placed under general anesthesia for the duration of the procedure. A midline incision is made on the scalp, and coordinates derived from skull landmarks&#8212;the bregma or lambda&#8212;are used to target the lateral ventricles for injection. Slow injection using an infusion pump delivers hemoglobin into the ventricle. This protocol is easy to use, versatile, and can model different components of IVH that result in PHH.

<table><tbody><tr><td>0.3 mL insulin syringe</td><td>BD Microfine + Insulin Syringe</td><td>230-4533</td><td>0.3-0.5 mL synringes will work</td></tr><tr><td>1.5 mL microtube</td><td>USA Scientific</td><td>1615-5500</td><td>Lot No. K194642H -3 511</td></tr><tr><td>4.7T MRI</td><td>Agilent/Varian</td><td>4.7T/33 cm</td><td>Agilent/Varian DirectDrive 4.7-T (200-MHz) MRI system</td></tr><tr><td>6-0 monofilament suture</td><td>ETHICON</td><td>667G</td><td></td></tr><tr><td>9.4T MRI</td><td>Bruker</td><td>BioSpec 94/20</td><td>Used in this protocol without the cryoprobe</td></tr><tr><td>Analytical balance</td><td>CCURIS Instruments</td><td>W3200-320</td><td></td></tr><tr><td>Artificial CSF (aCSF)</td><td>Tocris Bioscience</td><td>3525</td><td>Batch No: 72A</td></tr><tr><td>Betadine</td><td>Purdue Products L.P.</td><td>301005-00</td><td>NDC 67618-150-09</td></tr><tr><td>Carprofen (injectable)</td><td>Zoetis Inc.&amp;nbsp;</td><td>PI 4019448</td><td>Rimadyl</td></tr><tr><td>Ethanol</td><td>Decon Laboratories</td><td>2701</td><td></td></tr><tr><td>Heating pad</td><td>Sunbeam</td><td>E12107-819</td><td>UL 612A, Z-1228-001</td></tr><tr><td>Hemoglobin</td><td>MP Biomedicals</td><td>100714</td><td>LOT NO. SR02321</td></tr><tr><td>Isoflurane</td><td>Piramal Critical Care</td><td>NDC 66794-017-25</td><td></td></tr><tr><td>Isoflurane vaporizer</td><td>VETEQUIP</td><td>911103</td><td></td></tr><tr><td>Light for stereotactic insturment</td><td>Dolan-Jenner industries</td><td>Fiber-Lite MI-150</td><td></td></tr><tr><td>Microinjection syringe pump</td><td>World Precision Instruments</td><td>MICRO21</td><td>Serial 184034 T08K</td></tr><tr><td>MRI software</td><td>Bruker BioSpin</td><td>Paravision 360 3.2</td><td></td></tr><tr><td>Oxygen</td><td>Airgas Healthcare</td><td>UN1072</td><td>LOT NUMBER S1432080XA02</td></tr><tr><td>Sprague Dawley rats</td><td>Charles River Laboratories</td><td>Strain code: 001</td><td></td></tr><tr><td>Stereotactic instrument</td><td>KOPF Instuments</td><td>Model 900LS Lazy Susan</td><td></td></tr><tr><td>Sterile cotton tipped applicator</td><td>Fischerbrand</td><td>23-400-118</td><td></td></tr><tr><td>Surgical blade</td><td>covetrus</td><td>#10</td><td></td></tr><tr><td>Topical triple antibiotic</td><td>Triple Antibiotic Ointment</td><td>NDC 51672-2120-1</td><td></td></tr><tr><td>Ventricle volume quantification software</td><td>ITK-SNAP</td><td>ITK-SNAP 4.0.0 beta</td><td></td></tr></tbody></table>

modeling neonatal intraventricular hemorrhage through intraventricular injection of hemoglobin

Neonatal intraventricular hemorrhage (IVH) is a common consequence of premature birth and leads to brain injury, posthemorrhagic hydrocephalus (PHH), and lifelong neurological deficits. While PHH can be treated by temporary and permanent cerebrospinal fluid (CSF) diversion procedures (ventricular reservoir and ventriculoperitoneal shunt, respectively), there are no pharmacological strategies to prevent or treat IVH-induced brain injury and hydrocephalus. Animal models are needed to better understand the pathophysiology of IVH and test pharmacological treatments. While there are existing models of neonatal IVH, those that reliably result in hydrocephalus are often limited by the necessity for large-volume injections, which may complicate modeling of the pathology or introduce variability in the clinical phenotype observed.
Recent clinical studies have implicated hemoglobin and ferritin in causing ventricular enlargement after IVH. Here, we develop a straightforward animal model that mimics the clinical phenotype of PHH utilizing small-volume intraventricular injections of the blood breakdown product hemoglobin. In addition to reliably inducing ventricular enlargement and hydrocephalus, this model results in white matter injury, inflammation, and immune cell infiltration in periventricular and white matter regions. This paper describes this clinically relevant, simple method for modeling IVH-PHH in neonatal rats using intraventricular injection and presents methods for quantifying ventricle size post injection.

The success of injection was confirmed by radiologic&#160;and immunohistochemical means. Animals that underwent hemoglobin injection developed moderate acute ventriculomegaly when assessed via MRI (Figure 2A), with significantly larger lateral ventricles at 24 h and 72 h post hemoglobin injection compared to aCSF-injected animals (Figure 2B,C). While there was no significant difference in lateral ventricle volume between hemoglobin-injected and ...

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Modeling Neonatal Intraventricular Hemorrhage Through Intraventricular Injection of Hemoglobin

We present a model of neonatal intraventricular hemorrhage using rat pups that mimics the pathology seen in humans.

Neonatal intraventricular hemorrhage (IVH) is a common consequence of premature birth and leads to brain injury, posthemorrhagic hydrocephalus (PHH), and ...

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2.8K Views.  University of Kentucky. We present a model of neonatal intraventricular hemorrhage using rat pups that mimics the pathology seen in humans.

Video: Modeling Neonatal Intraventricular Hemorrhage Through Intraventricular Injection of Hemoglobin

Autologous Blood Injection to Model Spontaneous Intracerebral Hemorrhage in Mice

Investigation of the pathophysiology of injury after intracerebral
hemorrhage (ICH) requires a reproducible animal model. While ICH
accounts for 10-15% of all strokes, there remains no specific
effective therapy. The autologous blood injection model in mice
involves the stereotaxic injection of arterial blood into the basal
ganglia mimicking a spontaneous hypertensive hemorrhage in man. The
response to hemorrhage can then be studied in vivo and the
neurobehavioral deficits quantified, allowing for description of the
ensuing pathology and the testing of potential therapeutic agents. The
procedure described in this protocol uses the double injection
technique to minimize risk of blood reflux up the needle track, no
anticoagulants in the pumping system, and eliminates all dead space
and expandable tubing in the system.

The autologous blood injection model of intracerebral hemorrhage in mice described in this protocol uses the double injection technique to minimize risk of blood reflux up the needle track, no anticoagulants in the pumping system, and eliminates all dead space and expandable tubing in the system.

Investigation of the pathophysiology of injury after intracerebral
hemorrhage (ICH) requires a reproducible animal model.  While ICH
accounts for 10-15% ...

Modeling Intracerebral Hemorrhage in Mice: Injection of Autologous Blood or Bacterial Collagenase 

Spontaneous intracerebral hemorrhage (ICH) defines a potentially life-threatening neurological malady that accounts for 10-15% of all stroke-related hospitalizations and for which no effective treatments are available to date1,2. Because of the heterogeneity of ICH in humans, various preclinical models are needed to thoroughly explore prospective therapeutic strategies3. Experimental ICH is commonly induced in rodents by intraparenchymal injection of either autologous blood or bacterial collagenase4. The appropriate model is selected based on the pathophysiology of hemorrhage induction and injury progression. The blood injection model mimics a rapidly progressing hemorrhage. Alternatively, bacterial collagenase enzymatically disrupts the basal lamina of brain capillaries, causing an active bleed that generally evolves over several hours5. Resultant perihematomal edema and neurofunctional deficits can be quantified from both models. In this study, we described and evaluated a modified double injection model of autologous whole blood6 as well as an ICH injection model of bacterial collagenase7, both of which target the basal ganglia (corpus striatum) of male CD-1 mice. We assessed neurofunctional deficits and brain edema at 24 and 72 hr after ICH induction. Intrastriatal injection of autologous blood (30 &mu;l) or bacterial collagenase (0.075U) caused reproducible neurofunctional deficits in mice and significantly increased brain edema at 24 and 72 hr after surgery (p&lt;0.05). In conclusion, both models yield consistent hemorrhagic infarcts and represent basic methods for preclinical ICH research.

Modeling Intracerebral Hemorrhage in Mice: Injection of Autologous Blood or Bacterial Collagenase

Clinically relevant animal models of intracerebral hemorrhage (ICH) are needed to extend our knowledge of hemorrhagic stroke and to examine novel therapeutic strategies. In this study, we describe and evaluate two ICH models that implement unilateral injections of either autologous whole blood or bacterial collagenase into the basal ganglia (corpus striatum) of mice.

Spontaneous intracerebral hemorrhage (ICH) defines a potentially life-threatening neurological malady that accounts for 10-15% of all stroke-related ...

Medicine

Intrastriatal Injection of Autologous Blood or Clostridial Collagenase as Murine Models of Intracerebral Hemorrhage

Intracerebral hemorrhage (ICH) is a common form of cerebrovascular disease and is associated with significant morbidity and mortality. Lack of effective treatment and failure of large clinical trials aimed at hemostasis and clot removal demonstrate the need for further mechanism-driven investigation of ICH. This research may be performed through the framework provided by preclinical models. Two murine models in popular use include intrastriatal (basal ganglia) injection of either autologous whole blood or clostridial collagenase. Since, each model represents distinctly different pathophysiological features related to ICH, use of a particular model may be selected based on what aspect of the disease is to be studied. For example, autologous blood injection most accurately represents the brain&#39;s response to the presence of intraparenchymal blood, and may most closely replicate lobar hemorrhage. Clostridial collagenase injection most accurately represents the small vessel rupture and hematoma evolution characteristic of deep hemorrhages. Thus, each model results in different hematoma formation, neuroinflammatory response, cerebral edema development, and neurobehavioral outcomes. Robustness of a purported therapeutic intervention can be best assessed using both models. In this protocol, induction of ICH using both models, immediate post-operative demonstration of injury, and early post-operative care techniques are demonstrated. Both models result in reproducible injuries, hematoma volumes, and neurobehavioral deficits. Because of the heterogeneity of human ICH, multiple preclinical models are needed to thoroughly explore pathophysiologic mechanisms and test potential therapeutic strategies.

Preclinical models of intracerebral hemorrhage are utilized to mimic certain aspects of clinical disease. Thus, mechanisms of injury and potential therapeutic strategies may be explored. In this protocol, two models of intracerebral hemorrhage are described, intrastriatal (basal ganglia) injections of autologous blood or collagenase.

Intracerebral hemorrhage (ICH) is a common form of cerebrovascular disease and is associated with significant morbidity and mortality. Lack of effective ...

Intracerebroventricular and Intravascular Injection of Viral Particles and Fluorescent Microbeads into the Neonatal Brain

In the study on the pathogenesis of viral encephalitis, the infection method is critical. The first of the two main infectious routes to the brain is the hematogenous route, which involves infection of the endothelial cells and pericytes of the brain. The second is the intracerebroventricular (ICV) route. Once within the central nervous system (CNS), viruses may spread to the subarachnoid space, meninges, and choroid plexus via the cerebrospinal fluid. In experimental models, the earliest stages of CNS viral distribution are not well characterized, and it is unclear whether only certain cells are initially infected. Here, we have analyzed the distribution of cytomegalovirus (CMV) particles during the acute phase of infection, termed primary viremia, following ICV or intravascular (IV) injection into the neonatal mouse brain. In the ICV injection model, 5 &#181;l of murine CMV (MCMV) or fluorescent microbeads were injected into the lateral ventricle at the midpoint between the ear and eye using a 10-&#181;l syringe with a 27 G needle. In the IV injection model, a 1-ml syringe with a 35 G needle was used. A transilluminator was used to visualize the superficial temporal (facial) vein of the neonatal mouse. We infused 50 &#181;l of MCMV or fluorescent microbeads into the superficial temporal vein. Brains were harvested at different time points post-injection. MCMV genomes were detected using the in situ hybridization method. Fluorescent microbeads or green fluorescent protein expressing recombinant MCMV particles were observed by fluorescent microscopy. These techniques can be applied to many other pathogens to investigate the pathogenesis of encephalitis.

Here, we describe a simple method of intracerebroventricular and intravascular injection of viral particles or fluorescent microbeads into the neonatal mouse brain. The localization pattern of the virus and nanoparticles could be detected by microscopic evaluation or by in situ hybridization.

In the study on the pathogenesis of viral encephalitis, the infection method is critical. The first of the two main infectious routes to the brain is the ...

Massive Pontine Hemorrhage by Dual Injection of Autologous Blood

We provide a protocol to establish a massive pontine hemorrhage model in a rat. Rats weighing about 250 grams were used in this study. One hundred microliters of autologous blood was taken from the tail vein and stereotaxically injected into the pons. The injection process was divided into 2 steps: First, 10 &#181;L of blood was injected into a specific location, anteroposterior position (AP) -9.0 mm; lateral (Lat) 0 mm; vertical (Vert) -9.2 mm, followed by a second injection of the residual blood located at AP -9.0 mm; Lat 0 mm; Vert -9.0 mm with a 20-minute interval. The balance beam test, limb placement test, and the modified Voestch neuroscore were used to evaluate neurological function. Magnetic Resonance Imaging (MRI) was used to assess the volume of hemorrhage in vivo. The symptoms of this model were in line with patients with massive pontine hemorrhage.

We present a protocol to establish a massive pontine hemorrhage model in a rat via dual injection of autologous blood.

We provide a protocol to establish a massive pontine hemorrhage model in a rat. Rats weighing about 250 grams were used in this study. One hundred ...

Intravenous Injections in Neonatal Mice

Intravenous injection is a clinically applicable manner to deliver therapeutics. For adult rodents and larger animals, intravenous injections are technically feasible and routine. However, some mouse models can have early onset of disease with a rapid progression that makes administration of potential therapies difficult. The temporal (or facial) vein is just anterior to the ear bud in mice and is clearly visible for the first two days after birth on either side of the head using a dissecting microscope. During this window, the temporal vein can be injected with volumes up to 50 &#956;l. The injection is safe and well tolerated by both the pups and the dams. A typical injection procedure is completed within 1-2 min, after which the pup is returned to the home cage. By the third postnatal day the vein is difficult to visualize and the injection procedure becomes technically unreliable. This technique has been used for delivery of adeno-associated virus (AAV) vectors, which in turn can provide almost body-wide, stable transgene expression for the life of the animal depending on the viral serotype chosen.

Animal models of pediatric disease can experience early onset and aggressive disease progression. Clinically relevant therapy delivery to young mouse models can be technically difficult. This protocol describes a non-invasive intravenous injection method for newborn mice within the first two postnatal days of life.

Intravenous injection is a clinically applicable manner to deliver therapeutics. For adult rodents and larger animals, intravenous injections are ...

Biology

Intracranial Pressure Monitoring In Nontraumatic Intraventricular Hemorrhage Rodent Model

Survivors of intraventricular hemorrhage are often left with significant long-term memory impairment; thus, research utilizing intraventricular hemorrhage animal models is essential. In this study, we sought out ways to measure intracranial pressure, mean arterial pressure, and cerebral perfusion pressure during nontraumatic intraventricular hemorrhage in rats. The experimental design included three Sprague Dawley groups: sham, standard 200 &#181;l intraventricular hemorrhage, and vehicle control groups. By introducing an intraparenchymal fiberoptic pressure sensor, precise intracranial pressure measurements were obtained in all groups. Cerebral perfusion pressures were calculated with the knowledge of intracranial pressure and mean arterial pressure values. As expected, the intraventricular hemorrhage and vehicle control groups both experienced a rise in the intracranial pressure and subsequent decline in cerebral perfusion pressure during intraventricular injection of autologous blood and artificial cerebrospinal fluid, respectively. The addition of an intraparenchymal fiberoptic pressure sensor is beneficial in monitoring precise intracranial pressure changes.

Monitoring intracranial pressure in rodent&#160;models of nontraumatic intraventricular hemorrhage is not common in the current literature. Herein, we demonstrate a technique for measuring intracranial pressure, mean arterial pressure, and cerebral perfusion pressure during intraventricular hemorrhage in a rat&#160;animal model.

Survivors of intraventricular hemorrhage are often left with significant long-term memory impairment; thus, research utilizing intraventricular hemorrhage ...

A Neonatal Rodent Model of Retroorbital Vein Injection

Intravenous (iv) injection is the most used route of drug administration in neonates in the clinical setting. Therefore, retroorbital vein injection is an important method for compound administration in research, where successful proof-of-concept studies can progress into much-needed neonatal clinical trials. Most intravenous studies in neonatal rodents use the superficial temporal/facial vein. However, retroorbital injection becomes unreliable in neonatal rodents older than 2 days after the skin darkens and the vein is no longer visible. In the present protocol, we describe the retroorbital injection of the venous sinus in both the neonatal mouse and rat at ages when the superficial temporal vein is no longer visible, but the eyes have not opened yet. Eye-opening facilitates retro-orbital injection by enabling the researcher to clearly see that they are not perforating the eye when inserting the needle. We demonstrate that this technique can be performed in a reliable and reproducible manner without adverse effects. Additionally, we show that it can be used in many studies, such as administering compounds to study neonatal brain injury.

This protocol aims to demonstrate a reproducible venous administration route that can be used in rats and mice throughout the neonatal period. This procedure is important for preclinical rodent studies that wish to mirror drug administration in neonatal care units primarily using intravenous administration.

Intravenous (iv) injection is the most used route of drug administration in neonates in the clinical setting. Therefore, retroorbital vein injection is an ...

Description of a Swine Infant Model of Volume-Controlled Hemorrhagic Shock

Hemorrhagic shock is a leading cause of morbidity and mortality in pediatric patients. Interpretation of the clinical indicators validated in adults to guide resuscitation and comparison between different therapies is difficult in children due to the inherent heterogeneity of this population. As a result, compared to adults, appropriate management of pediatric hemorrhagic shock is still not well established. In addition, the scarcity of pediatric patients with hemorrhagic shock precludes the development of clinically relevant studies. For this reason, an experimental pediatric animal model is necessary to study the effects of hemorrhage in children as well as their response to different therapies. We present an infant animal model of volume-controlled hemorrhagic shock in anesthetized young pigs. Hemorrhage is induced by withdrawing a previously calculated blood volume, and the pig is subsequently monitored and resuscitated with different therapies. Here, we describe a precise and highly reproducible model of hemorrhagic shock in immature swine. The model yields hemodynamic data that characterizes compensatory mechanisms that are activated in response to severe hemorrhage.

This article aims to provide researchers with a detailed and accessible guide to set up an infant porcine model of hemorrhagic shock.

Hemorrhagic shock is a leading cause of morbidity and mortality in pediatric patients. Interpretation of the clinical indicators validated in adults to ...

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 ...

Modeling Neonatal Intraventricular Hemorrhage Through Intraventricular Injection of Hemoglobin

Podsumowanie

Przeglądaj więcej filmów

Autologous Blood Injection to Model Spontaneous Intracerebral Hemorrhage in Mice

Modeling Intracerebral Hemorrhage in Mice: Injection of Autologous Blood or Bacterial Collagenase

Intrastriatal Injection of Autologous Blood or Clostridial Collagenase as Murine Models of Intracerebral Hemorrhage

Intracerebroventricular and Intravascular Injection of Viral Particles and Fluorescent Microbeads into the Neonatal Brain

Massive Pontine Hemorrhage by Dual Injection of Autologous Blood

Intravenous Injections in Neonatal Mice

Intracranial Pressure Monitoring In Nontraumatic Intraventricular Hemorrhage Rodent Model

A Neonatal Rodent Model of Retroorbital Vein Injection

Description of a Swine Infant Model of Volume-Controlled Hemorrhagic Shock

Modeling Posthemorrhagic Hydrocephalus of Prematurity in Rats