A Grant Mérito do Departamento de Assuntos de Veteranos e uma bolsa T32-HL098062 do NHLBI dos Institutos Nacionais de Saúde apoiaram este trabalho. Queremos agradecem o conselho de Randolph H. Hasting, MD, Ph.D. e os conselhos e apoio da Unidade de Medicina Veterinária do Sistema de Saúde VA San Diego.

1. Preparação animal <ol><li> Obter ratos que estão com mais de 8 semanas e mais de 20 g (camundongos menores podem ser entubado por um especialista). </li><li> Anestesia <ol><li> Injectar ratinhos com 20 mg / kg, cada uma, de cetamina e xilazina intraperitonealmente como uma pré-anestésica. (Esta dose é insuficiente para anestesiar totalmente o mouse, mas facilita a transferência, após intubação, a ventilação mecânica.) No entanto, o ajuste das doses podem ser necessárias de acordo com a resposta do anestésico, em consulta com o veterinário institucional.) </li><li> Induzir a anestesia em ratos com 3,5% de isoflurano / oxigênio em uma câmara de indução para 90-120 seg. </li><li> Observar a freqüência respiratória com cuidado. Deve diminuir progressivamente a não menos de 45 bpm. </li></ol></li></ol> 2. Preparação para intubação <ol><li> Remover o rato da câmara de indução e nuca com força. </li><li> Use uma pinça fina almofadadas a gently estender a língua da boca. </li><li> Manter extensão da língua, segurando a língua entre dois dedos e aplicar a força suave. </li><li> Puxe o mouse em cima da espéculo do otoscópio com um movimento vertical. </li><li> Olhe pela ocular do otoscópio enquanto scruffing firmemente e puxe o mouse para cima suavemente pela língua e da nuca. </li><li> Olhe atentamente para as cordas vocais. Eles devem ser facilmente visíveis neste momento. O aditus laryngis (a estrutura da abertura da laringe) deve parecer relativamente branco. Não deve haver movimento dos cordões, com cada respiração. Se os cabos não estão se movendo ou são mal visualizado, gire o animal um pouco e delicadamente hiperextensão do pescoço. </li><li> Com a mão dominante, segure a 20 G, 1 em cateter, com um comprimento de um centímetro do tubo PE10 se estende através da ponta do cateter, como um lápis e coloque-o ao lado do espéculo. O tubo de PE serve como um estilete ou vela. </li><li> Direcione a tubi PE10ng (estilete) através das cordas vocais e avançar o cateter de 20 G (tubo endotraqueal) sobre o tubo de PE, até o cubo está ao nível dos incisivos inferiores. Remover esta estilete rapidamente. </li><li> Delicadamente, levar o animal fora do espéculo e verificar a localização do tubo, colocando o animal em um ventilador mecânico com contínua isoflurano a 2% para manter a anestesia geral durante todo o experimento. Visualize ar expirado (bolhas) passando por uma armadilha PEEP para confirmar a intubação. Embora prótese esofágica pode resultar em algumas bolhas, não será tão pronunciados ou como consistente com a intubação endotraqueal. Além disso, observar um traçado da pressão das vias aéreas para desvios negativos (Figura 1). Estes confirmar o posicionamento adequado do tubo. Alternativamente, coloque uma pequena quantidade de água em tubos IV e conectá-lo ao tubo ET. Verificando o movimento de e para o mouse com a respiração 2. No caso da prótese esofágica, do prastreamento ressure revelará pressões significativamente mais elevados e sem desvios negativos. Embora ao final da expiração de CO 2 seria útil, tecnicamente isso seria muito difícil, dado os pequenos volumes correntes (~ 200 mL) e o equipamento para fazer isso seria muito caro. As técnicas simples descritas são inteiramente suficiente e muito menos dispendioso. Se a anestesia de isoflurano não está disponível, todos os procedimentos podem ser realizados utilizando cetamina 80-120 mg / kg em conjunto com xilazina 10-20 mg / kg de anestesia geral. </li></ol> 3. Técnica Alternativa: laringoscopia direta com a Técnica otoscópio é usado Prontamente para outros fins, principalmente para o direto instilação de substâncias estudo sobre o pulmão. <ol><li> Induzir a anestesia dos animais com isoflurano sozinho para este procedimento em 3,5% de 90-120 segundos na câmara de indução. </li><li> Nuca do animal com força na base do crânio e estender a língua suavementecom uma pinça fina. </li><li> Segurando a língua gentilmente, puxe o animal para cima sobre o espéculo (sem modificações) até que o animal não pode ser puxado para cima ainda mais. </li><li> As cordas vocais podem ser visualizados na maioria das vezes por esta técnica por si só, mas girar o animal e hiper-estendeu o pescoço para trazê-los em plena vista. </li><li> Avance uma pipeta de gel de carregamento contendo o instilado a glote e incutir o fluido. Porque o espéculo faz um selo com a hipofaringe o mouse irá aspirar qualquer líquido residual que não atravessa as cordas. Este é facilmente verificado pelo rhonchorous soa o rato torna agora quando a respiração até que o fluido é distribuído completamente nos pulmões. </li><li> Em alternativa, ligar PE10 tubagem para uma seringa de 0,5 ml contendo 50 ul de fluido com um bolus de ar atrás do líquido. Avançar o tubo PE cuidadosamente através das cordas vocais para 0,5 cm e descarregar o conteúdo para a via aérea lentamente. No entanto, o trauma ocasional para as vias aéreas inferiores ocorre ucantar esta técnica sem a melhor entrega da amostra. </li></ol>

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Os autores declaram que não têm interesses financeiros concorrentes.

Neste relatório nós descrevemos uma técnica simples e confiável para entubar ratos que é não traumática e pode ser usado repetidamente no mesmo animal. Esta técnica pode ser realizada com laboratório simples ou equipamentos médicos que podem ser comprados por uma módica quantia. A técnica de laringoscopia directa, originalmente relatado por Hastings e colegas 4, pode também ser usado para uma variedade de fins, mas principalmente para administrar com precisão as substâncias de ensaio para o tra...

O rato de laboratório suplantou praticamente todas as espécies como o principal modelo de mamíferos de biologia e pathobiology. O rato de laboratório é a menor espécie de mamíferos que tem sido clara e exaustivamente demonstrado ser de valor como um modelo da doença humana e provou inestimável em avanços de nossa compreensão da biologia humana e doenças. O tempo de gestação curto e substancialmente menor custo tem permitido o desenvolvimento e estudo de ratinhos nulos e transgénicos como uma ferramenta comum em pesquisa biomédica. No entanto, o tamanho do rato de laboratório média (20-25 g) tem limitado o seu estudo em estudos com base fisiológica ou cirurgicamente e, consequentemente, alguns investigadores estudar espécies de mamíferos maiores. Um impedimento ao uso de camundongos nestes estudos é a dificuldade encontrada com técnicas de intubação que permitiriam medidas fisiológicas ou extensos procedimentos cirúrgicos sob anestesia profunda. Traqueostomia 1 tem sido utilizado como um padrão de tehaver descrição prévia em vez de intubação, devido à maior facilidade de realizar esta técnica e habilidade modesto necessário. No entanto, a traqueostomia não é propício para estudos de cirurgia, crônicas ou de recuperação; Assim, é limitada a experiências agudas. A traqueostomia também pode ser uma variável de confusão na pesquisa em que a inflamação ou reflexos fisiológicos sensíveis são importantes. O nosso laboratório tem tentado a maioria das técnicas descritas por outros investigadores e encontrou-inadequada para uma variedade de razões. A traqueostomia é muito traumático e induz a sangramento e inflamação das vias aéreas. Muito mais problemático é que ele não pode ser viável repetido. Muitas técnicas relativamente não invasivos que requerem um investimento modesto em equipamentos não são suficientemente fiáveis. Outras técnicas exigem equipamentos caros que é difícil de justificar, sem saber se o equipamento irá trabalhar em um aplicativo específico. Assim, buscou-se desenvolver uma técnica não traumática que não necessitaram de mais than um pequeno investimento em equipamento especializado, pode ser conseguida rapidamente e de forma fiável, pode ser repetido em modelos crónicos, e poderia ser utilizada em um grande número de animais. Aqui nós relatamos tal técnica.

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			<td height="17" style="height:17px;width:411px;">Operating Otoscope Head</td>
			<td style="width:144px;">Welch Allyn</td>
			<td align="right" style="width:83px;">21700</td>
			<td style="width:69px;">&#160;$188.98</td>
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		<tr height="17">
			<td height="17" style="height:17px;">Otoscope Handle</td>
			<td>Welch Allyn</td>
			<td align="right">71000</td>
			<td>&#160;$112.20</td>
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			<td height="17" style="height:17px;">Reuseable Speculum</td>
			<td>Welch Allyn</td>
			<td align="right">22002</td>
			<td>&#160;$ 3.98</td>
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			<td height="17" style="height:17px;">Fine Forceps</td>
			<td>Miltex</td>
			<td>18-779</td>
			<td>&#160;$107.18</td>
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			<td height="17" style="height:17px;">Small clamp stand to hold otoscope</td>
			<td></td>
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			<td height="17" style="height:17px;">Isoflurane Vaporizer (multiple circuit with vacuum waste gas handling)</td>
			<td>Summit Medical</td>
			<td></td>
			<td align="right">$3,000</td>
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			<td height="17" style="height:17px;">Flexivent (Animal Ventilator)</td>
			<td>SCIREQ</td>
			<td></td>
			<td align="right">$35,000</td>
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			<td></td>
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			<td height="17" style="height:17px;">Supplies</td>
			<td></td>
			<td></td>
			<td></td>
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		<tr height="17">
			<td height="17" style="height:17px;">Intravenous catheter (20 ga x 1 inch)</td>
			<td>BD</td>
			<td align="right">381233</td>
			<td>&#160;$&#160; 9.62</td>
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			<td height="17" style="height:17px;">Polyethylene tubing (PE10) (0.011 inch I.D., 0.024 inch O.D.) 100 ft</td>
			<td>Intramedic, Clay-Adams</td>
			<td align="right">427401</td>
			<td>&#160;$115.70</td>
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		<tr height="17">
			<td height="17" style="height:17px;">Ketamine 100 mg/ml (10 ml bottle)</td>
			<td>Butler</td>
			<td align="right">23061</td>
			<td>&#160;$10.00</td>
		</tr>
		<tr height="17">
			<td height="17" style="height:17px;">Xylazine (100 ml bottle)</td>
			<td>Vedco</td>
			<td align="right">24105</td>
			<td>&#160;$20.00</td>
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			<td height="17" style="height:17px;">Isoflurane (250 ml bottle)</td>
			<td></td>
			<td></td>
			<td>&#160;$15.00</td>
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		<tr height="17">
			<td height="17" style="height:17px;">vecuronium bromide 10 mg/10 ml</td>
			<td>Pfizer</td>
			<td>NDC 0069-0094-01</td>
			<td align="right">$15.00</td>
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endotracheal intubation in mice via direct laryngoscopy using an otoscope

Ratos, ambos do tipo selvagem e transgênica, são o modelo de mamíferos capital em pesquisa biomédica atualmente. Intubação e ventilação mecânica são necessários para experimentos com animais inteiros que necessitam de cirurgia sob anestesia profunda ou medidas de função pulmonar. A traqueostomia tem sido o padrão para entubar as vias aéreas nestes ratos para permitir a ventilação mecânica. A entubação orotraqueal foi relatado, mas não tem sido utilizada com sucesso em muitos estudos, devido à dificuldade técnica substancial ou uma necessidade de equipamento altamente especializado e caro. Aqui nós relatamos uma técnica de laringoscopia direta utilizando um otoscópio equipado com um espéculo 2,0 mm e com um cateter intravenoso 20 G como um tubo endotraqueal. Nós temos usado esta técnica extensivamente e de forma confiável para entubar e realizar avaliações precisas da função pulmonar em camundongos. Esta técnica tem se mostrado segura, com praticamente nenhuma perda de animais em mãos experientes. Além disso, esta técnicapode ser utilizado para estudos repetidos de ratinhos em modelos crónicos.

Intubação com a técnica acima é confiável e rápido. O posicionamento adequado do tubo endotraqueal é mais facilmente verificado observando borbulhamento de gases expirados a partir do membro expiratório submersa do circuito do ventilador (geralmente numa armadilha de PEEP) e desvios negativos sobre a pressão das vias respiratórias traçando (Figura 1). Os desvios negativos sobre o rastreamento de pressão nas vias aéreas são as mais confiáveis. Outros têm utilizado o movimento de uma peque...

Watch this Scientific Journal Video about Endotracheal Intubation in Mice via Direct Laryngoscopy Using an Otoscope at JoVE.com

Endotracheal Intubation in Mice via Direct Laryngoscopy Using an Otoscope

Nós desenvolvemos um método simples, confiável e relativamente barata para a intubação traqueal em ratos através de laringoscopia direta utilizando um otoscópio com um espéculo 2,0 mm. Esta técnica é não traumático e pode ser usado para as medições repetidas em experiências crónicas. Achamos superior à traqueostomia ou relatado anteriormente técnicas não cirúrgicas.

Entubação endotraqueal em Ratos<em&gt; Via</em&gt; Laringoscopia direta Usando um otoscópio

Mice, both wildtype and transgenic, are the principal mammalian model in biomedical research currently. Intubation and mechanical ventilation are ...

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Endotracheal Intubation in Mice via Direct Laryngoscopy Using an Otoscope

30.8K visualizações.  VA San Diego Healthcare System.  Nós desenvolvemos um método simples, confiável e relativamente barata para a intubação traqueal em ratos através de laringoscopia direta utilizando um otoscópio com um espéculo 2,0 mm. Esta técnica é não traumático e pode ser usado para as medições repetidas em experiências crónicas. Achamos superior à traqueostomia ou relatado anteriormente técnicas não cirúrgicas. 

Vídeo: Endotracheal Intubation in Mice via Direct Laryngoscopy Using an Otoscope

Using Quantitative Real-time PCR to Determine Donor Cell Engraftment in a Competitive Murine Bone Marrow Transplantation Model

Murine bone marrow transplantation models provide an important tool in measuring hematopoietic stem cell (HSC) functions and determining genes/molecules that regulate HSCs. In these transplant model systems, the function of HSCs is determined by the ability of these cells to engraft and reconstitute lethally irradiated recipient mice. Commonly, the donor cell contribution/engraftment is measured by antibodies to donor- specific cell surface proteins using flow cytometry. However, this method heavily depends on the specificity and the ability of the cell surface marker to differentiate donor-derived cells from recipient-originated cells, which may not be available for all mouse strains. Considering the various backgrounds of genetically modified mouse strains in the market, this cell surface/ flow cytometry-based method has significant limitations especially in mouse strains that lack well-defined surface markers to separate donor cells from congenic recipient cells. Here, we reported a PCR-based technique to determine donor cell engraftment/contribution in transplant recipient mice. We transplanted male donor bone marrow HSCs to lethally irradiated congenic female mice. Peripheral blood samples were collected at different time points post transplantation. Bone marrow samples were obtained at the end of the experiments. Genomic DNA was isolated and the Y chromosome specific gene, Zfy1, was amplified using quantitative Real time PCR. The engraftment of male donor-derived cells in the female recipient mice was calculated against standard curve with known percentage of male vs. female DNAs. Bcl2 was used as a reference gene to normalize the total DNA amount. Our data suggested that this approach reliably determines donor cell engraftment and provides a useful, yet simple method in measuring hematopoietic cell reconstitution in murine bone marrow transplantation models. Our method can be routinely performed in most laboratories because no costly equipment such as flow cytometry is required.

Determining donor cell engraftment presents a challenge in mouse bone marrow transplant models that lack well-defined phenotypical markers. We described a methodology to quantify male donor cell engraftment in female transplant recipient mice. This method can be used in all mouse strains for the study of HSC functions.

Usando Quantitative PCR em tempo real para determinar enxerto célula dadora num modelo murino de osso Competitiva Marrow Transplantation

Murine bone marrow transplantation models provide an important tool in measuring hematopoietic stem cell (HSC) functions and determining genes/molecules ...

Medicina

A Simple Method of Mouse Lung Intubation

A simple procedure to intubate mice for pulmonary function measurements would have several advantages in longitudinal studies with limited numbers or expensive animal. One of the reasons that this is not done more routinely is that it is relatively difficult, despite there being several published studies that describe ways to achieve it. In this paper we demonstrate a procedure that eliminates one of the major hurdles associated with this intubation, that of visualizing the trachea during the entire time of intubation. The approach uses a 0.5 mm fiberoptic light source that serves as an introducer to direct the intubation cannula into the mouse trachea. We show that it is possible to use this procedure to measure lung mechanics in individual mice over a time course of at least several weeks. The technique can be set up with relatively little expense and expertise, and it can be routinely accomplished with relatively little training. This should make it possible for any laboratory to routinely carry out this intubation, thereby allowing longitudinal studies in individual mice, thereby minimizing the number of mice needed and increasing the statistical power by using each mouse as its own control.

This paper describes a striaghforward and efficient method of intubating mice for pulmonary function measurements or pulmonary instillation, that allows the mice to recover and be studied at later times. The procedure involves an inexpensive fiberoptic light source that directly illuminates the trachea.

Um método simples de intubação Lung Rato

A  simple procedure to intubate mice for pulmonary function measurements would  have several advantages in longitudinal studies with limited numbers or  ...

Heterotopic Mucosal Engrafting Procedure for Direct Drug Delivery to the Brain in Mice

Delivery of therapeutics into the brain is impeded by the presence of the blood-brain barrier (BBB) which restricts the passage of polar and high molecular weight compounds from the bloodstream and into brain tissue. Some direct delivery success in humans has been achieved via implantation of transcranial catheters; however this method is highly invasive and associated with numerous complications. A less invasive alternative would be to dose the brain through a surgically implanted, semipermeable membrane such as the nasal mucosa that is used to repair skull base defects following endoscopic transnasal tumor removal surgery in humans. Drug transfer though this membrane would effectively bypass the BBB and diffuse directly into the brain and cerebrospinal fluid. Inspired by this approach, a surgical approach in mice was developed that uses a donor septal mucosal membrane engrafted over an extracranial surgical BBB defect. This model has been shown to effectively allow the passage of high molecular weight compounds into the brain. Since numerous drug candidates are incapable of crossing the BBB, this model is valuable for performing preclinical testing of novel therapies for neurological and psychiatric diseases.

A mouse model of human endoscopic skull base reconstruction has been developed that creates a semipermeable interface between the brain and nose using nasal mucosal grafts. This method allows researchers to study delivery to the central nervous system of high molecular weight therapeutics which are otherwise excluded by the blood-brain barrier when administered systemically.

Heterotópico mucosa enxertando Procedimento para entrega da droga direto para o cérebro em ratos

Delivery of therapeutics into the brain is impeded by the presence of the blood-brain barrier (BBB) which restricts the passage of polar and high ...

An Improved Method for Rapid Intubation of the Trachea in Mice

Despite some anatomical and physiological differences, mouse models continue to be an essential tool for studying human lung disease. Bleomycin toxicity is a commonly used model to study both acute lung injury and fibrosis, and multiple methods have been developed for administering bleomycin (and other toxic agents) into the lungs. However, many of these approaches, such as transtracheal instillation, have inherent drawbacks, including the need for strong anesthetics and survival surgery. This paper reports a quick, reproducible method of intratracheal intubation that involves mild inhaled anesthesia, visualization of the trachea, and the use of a surrogate spirometer to confirm exposure. As a proof of concept, 8-12 week old C57BL/6 mice were administered either 2.0 U/kg of bleomycin or an equivalent volume of PBS, and both damage and fibrotic endpoints were measured post-exposure. This procedure allows researchers to treat a large cohort of mice in a relatively short period with little expense and minimal post-procedure care.

This article presents a rapid and simple method for administering bleomycin directly into the mouse trachea via intubation. Key advantages of this method are that it is highly reproducible, easy to master, and does not require specialized equipment or lengthy recovery times.

Um método melhorado para rápida de intubação da traqueia em Ratos

Despite some anatomical and physiological differences, mouse models continue to be an essential tool for studying human lung disease. Bleomycin toxicity ...

Inducing Acute Lung Injury in Mice by Direct Intratracheal Lipopolysaccharide Instillation

Airway administration of lipopolysaccharide (LPS) is a common way to study pulmonary inflammation and acute lung injury (ALI) in small animal models. Various approaches have been described, such as the inhalation of aerosolized LPS as well as nasal or intratracheal instillation. The presented protocol describes a detailed step-by-step procedure to induce ALI in mice by direct intratracheal LPS instillation and perform FACS analysis of blood samples, bronchoalveolar lavage (BAL) fluid, and lung tissue. After intraperitoneal sedation, the trachea is exposed and LPS is administered via a 22 G venous catheter. A robust and reproducible inflammatory reaction with leukocyte invasion, upregulation of proinflammatory cytokines, and disruption of the alveolo-capillary barrier is induced within hours to days, depending on the LPS dosage used. Collection of blood samples, BAL fluid, and lung harvesting, as well as the processing for FACS analysis, are described in detail in the protocol. Although the use of the sterile LPS is not suitable to study pharmacologic interventions in infectious diseases, the described approach offers minimal invasiveness, simple handling, and good reproducibility to answer mechanistic immunological questions. Furthermore, dose titration as well as the use of alternative LPS preparations or mouse strains allow modulation of the clinical effects, which can exhibit different degrees of ALI severity or early vs. late onset of disease symptoms.

Presented here is a step-by-step procedure to induce acute lung injury in mice by direct intratracheal lipopolysaccharide instillation and to perform FACS analysis of blood samples, bronchoalveolar lavage fluid, and lung tissue. Minimal invasiveness, simple handling, good reproducibility, and titration of disease severity are advantages of this approach.

Induzindo lesão pulmonar aguda em camundongos por instilação de lipopolissacárido intratraqueal direto

Airway administration of lipopolysaccharide (LPS) is a common way to study pulmonary inflammation and acute lung injury (ALI) in small animal models. ...

Repeated Orotracheal Intubation in Mice

The literature describes several methods for mouse intubation that either require visualization of the glottis through the oral cavity or incision in the ventral neck for direct confirmation of cannula placement in the trachea. The relative difficulty or the tissue trauma induced to the subject by such procedures can be an impediment to an investigator&#8217;s ability to perform longitudinal studies. This article illustrates a technique in which physical manipulation of the mouse following the use of a depilatory to remove hair from the ventral neck permits transcutaneous visualization of the trachea for orotracheal intubation regardless of degree of skin pigmentation. This method is innocuous to the subject and easily achieved with a limited understanding of murine anatomy. This refined approach facilitates repeated intubation, which may be necessary for monitoring progression of disease or instillation of treatments. Using this method may result in a reduction of the number of animals and technical skill required to measure lung function in mouse models of respiratory disease.

The goal of this article is to describe a refined method of intubation of the laboratory mouse. The method is noninvasive and, therefore, ideal for studies that require serial monitoring of respiratory function and/or instillation of treatments into the lung.

Intubação Orotraqueal Repetida em Camundongos

The literature describes several methods for mouse intubation that either require visualization of the glottis through the oral cavity or incision in the ...

Blind Endotracheal Intubation in Neonatal Rabbits

The newborn rabbit is a useful animal model for various pathologies and procedures. Airway management of the rabbit is complex due to its anatomical characteristics, which is further complicated in the case of the newborn. Of the different methods of advanced airway management, endotracheal intubation is less aggressive than tracheostomy, and is more feasible than supraglottic management given the lack of supraglottic devices of such a small size. As direct glottis visualization is very difficult in animals this size, this blind intubation model is presented as an effective alternative, especially for experiments requiring prolonged anesthesia. Using this method, we performed blind intubations with a 90% success rate.

We describe a technique of endotracheal intubation in newborn rabbits after esophageal catheterization with a gastric tube.

Intubação endotraqueal cega em coelhos neonatais

The newborn rabbit is a useful animal model for various pathologies and procedures. Airway management of the rabbit is complex due to its anatomical ...

Direct Drug Delivery to Kidney via the Renal Artery

There is a need for directed injections to enable increased and specific renal exposure for efficient evaluation of drug targets in the renal research field. Accumulation of drugs in certain organs may give rise to adverse and unwanted effects, depending on the nature of injectate. To minimize spillover and/or accumulation in other tissues, the herein described method directs the formulation into the renal artery bloodstream by inserting a catheter in the infra renal aorta, just below where it branches into the renal artery, resulting in the kidney as first reached organ and distributing of formulation throughout the kidney.
This manuscript provides a detailed description of the method, as well as its challenges and difficulties. It guides the experimenter to become skillful with this type of microsurgery that requires accuracy under sterile conditions. Speed is crucial for minimizing the ischemia and practicing the procedure will increase the chance of successful injections without adverse effects. By modulating the time between injection and reperfusion as well as the injected volume, the risk of spillover to other organs is mitigated. 
Note that this technique is suitable for single dosing strategies.

This manuscript describes a method for targeted delivery to a single kidney via a catheter placed in the infrarenal abdominal aorta in the mouse.

Entrega direta de medicamentos ao rim através da artéria renal

There is a need for directed injections to enable increased and specific renal exposure for efficient evaluation of drug targets in the renal research ...

Endotracheal Intubation Using a Flexible Intubation Endoscope as a Standardized Model for Safe Airway Management in Swine

Endotracheal intubation is often a basic requirement for translational research in porcine models for various interventions that require a secured airway or high ventilation pressures. Endotracheal intubation is a challenging skill,&#160;requiring a minimum number of successful endotracheal intubations to achieve a high success rate under optimal conditions, which is often unachievable for non-anaesthesiology researchers. Due to the specific porcine airway anatomy, a difficult airway can usually be assumed. The impossibility of establishing a secure airway can result in injury, adverse events, or death of the laboratory animal. Using a prospective, randomized, controlled evaluation approach, it has been shown that fiberoptic-assisted endotracheal intubation takes longer but has a higher first-pass success rate than conventional intubation without causing clinically relevant drops in oxygen saturation. This model presents a standardized regimen for endoscopically guided endotracheal intubation, providing a secured airway, especially for researchers who are inexperienced in the technique of endotracheal intubation via direct laryngoscopy. This procedure is expected to minimize animal suffering and unnecessary animal losses.

The use of pigs in research has increased in recent years. Nevertheless, pigs are characterized by difficult airway anatomy. By demonstrating how to perform endoscopically guided endotracheal intubation, the present protocol aims to further increase laboratory animals' safety to avoid animal suffering and unnecessary death.

Intubação endotraqueal usando um endoscópio de intubação flexível como modelo padronizado para o manejo seguro das vias aéreas em suínos

Endotracheal intubation is often a basic requirement for translational research in porcine models for various interventions that require a secured airway ...

<meta charset="utf8"></head><body>Protocolo de intubação endotraqueal baseado em traqueotomia para modelos de ratos não sobreviventes

Endotracheal Intubation via Tracheotomy and Subsequent Thoracotomy in Rats for Non-Survival Applications

Endotracheal intubation and subsequent ventilation are often basic requirements for translational research in rat models for various interventions that require controlled or high ventilation pressures or access to the thoracic cavity and organs. Conventional endoorotracheal intubation using the anatomically existing route through the mouth is well suited for survival experiments. However, this procedure poses some challenges, including generally higher levels of the required experience and technical skill, more advanced equipment, and greater time effort with relevant intubation failure rates and complications such as tracheal perforation, temporary systemic hypooxygenation, and relevant aerial leakage.
This manuscript, therefore, presents a detailed step-by-step protocol for endotracheal intubation through tracheotomy in non-survival rat models when guaranteed intubation success, constant oxygenation levels, high ventilation pressures, or open thoracotomy are required.
The protocol emphasizes the importance of meticulous surgical technique to ensure consistent and reliable outcomes, especially for researchers who are inexperienced or lack routine in the technique of endoorotracheal intubation via direct laryngoscopy. This procedure is, therefore, expected to minimize animal suffering and unnecessary animal losses.

<meta charset="utf8"></head><body>Intubação endotraqueal via traqueotomia e subsequente toracotomia em ratos para aplicações de não sobrevivência

Here we introduce a standardized procedure for endotracheal intubation via tracheotomy followed by thoracotomy in rats, aimed at enhancing the precision and reproducibility of non-survival applications requiring invasive ventilation and exposure of thoracic organs in in vivo rat models.

Intubação endotraqueal via traqueotomia e subsequente toracotomia em ratos para aplicações de não sobrevivência

Endotracheal intubation and subsequent ventilation are often basic requirements for translational research in rat models for various interventions that ...