The authors would like to acknowledge the Cincinnati Children&#8217;s Hospital Division of Veterinary Services for their assistance. This manuscript was supported by the National Institutes of Health K12 HD028827. Anna Perl PhD taught the authors this surgical procedure.

NOT: Hayvan kullanım bildirimi: Bu çalışmada tüm işlemler onay ve Cincinnati Çocuk Hastanesi Kurumsal Hayvan Kullanımı ve Bakımı Komitesi (IACUC) yönergeleri takip gerçekleştirilmiştir. Sekiz hafta yaşında C57BL / 6J erkek fareleri, Jackson Laboratories&#39;den (Bar Harbor, ME) elde edilir ve kullanımdan önce bir hafta boyunca ortama alışmaları sağlandı. Cerrahi kadar, hayvanlar patojen madde içermeyen bir yere yerleştirilmesi ve otoklavlanmıştır yemi ve süzüldü suyu ad libdium sağlandı. Her fare kafesi özel hava ve su ile sağlanan ve odalar 12 saat gece-gündüz döngüsü tutuldu. Cerrahi işlemden sonra, fareler, süzüldü üstleri ile kafeslerde muhafaza otoklavlanmış yemi farelere istenildiği kadar mesafede, ve bir su şişesinden su süzüldü sağlandı. Araçların 1. Hazırlık <ol><li> Ataç ve işaretçilerine kullanılarak 6 cilt Ekartörleri olun. Büküm kağıt pim Shanks üzerine ataç doğruldu, lbir ucunda bir 5 cm&#39;lik tek bir çelik tel eave ve telin ucunda tek bir 0.5 cm&#39;lik bir &quot;U&quot; şekilli bir kancayı olun. </li><li> Plastik wrap kullanarak bazı 15 x 15 cm kare cerrahi perdeler olun. Fare başına bir pansuman hazırlayın. Her şal arasında bir kağıt kule koyun. </li><li> 12 x 12 inç mantar fayans, gazlı bez ve pamuklu çubuklar bir yığını ile birlikte tüm cerrahi aletler sterilize. </li></ol> 2. Fare Hazırlama <ol><li> % 2 izofluran ile anestezi neden olur. Hayvan tartılır. </li><li> Özel cerrahi hazırlık alanında elektrik tıraş sol toraks ve boyun alanı tıraş. </li><li> Farenin gözlerine yapay gözyaşı merhemi bir damla uygulayın. </li><li> Klorheksidin ve izopropil alkol ile boyun ve sol toraks arındırın. Iki kez daha tekrarlayın. </li></ol> 3. Fare Oro-trakeal entübasyon ve Mekanik Ventilasyon <ol><li> Steril olmayan bir cerrahi teknisyen yerde önceden ısıtılmış cerrahi alanında fare sırtüstü var.</li><li> Pençe tutam yanıt eksikliği belgeleyerek anestezi derinliği onaylayın. </li><li> Cerrahi kıyafetleri, maske, şapka ve ellerini yıkama ve donning sonra, steril cerrahi eldiven yok. </li><li> Dökümlü ve aseptik teknik kullanılarak sonra, gırtlak maruz ön orta boyun üzerinde 1 cm&#39;lik dikey kesi yapmak. Hafif kavisli, tırtıklı 10 cm forseps ile kayış kasları geri çekin ve düz makas ucu ile kayış kasları yayarak gırtlak ve trakea maruz. </li><li> Oral orta trakea (Şekil 1A) içine 22 G künt uçlu angiocatheter yerleştirin ve görsel yerleştirme (Şekil 1B) onaylayın. Anestezi koruyun ve kemirgen ventilatör ile (inme başına 225 ul; min başına 200 Stokes)% 1-3 izofluran kullanarak havalandırın. 15 cm H2O bir basınç sınırını ayrılmadan </li></ol> 4. Fare Pnömonektomi <ol><li> Farenin arka bakacak sağ lateral dekübit pozisyonunda fare LayOperatör (sol taraf yukarı). Steril örtü olarak kendi kendine kapanan plastik wrap kullanın. Drape ile kesme, 4. ve 5. interkostal aralıktan kaburga 2 cm uzunluğunda kesilmiş paralel hale getirmek için künt uçlu kavisli makas kullanın. Kör uç kavisli makas yerleştirin ve alttaki kaburga ve interkostal kasların uzak cildi teşrih. </li><li> Bir kare 1.5 x 1.5 cm cerrahi pencere (Şekil 2A) maruz dört toplayıcıları ile cildi geri çekin. Mantar kuruluna Ekartörleri sabitleyin. </li><li> Kavisli bir forseps kullanarak kaburga aşağı incelemek ve göğüs boşluğu girmek için kavisli bir forseps bir ucunu kullanın. </li><li> Künt ucu mikro-makas kullanarak, göğüs boşluğu girmek için alt bıçak kullanın. Ters yönde kaburga ve tekrarı arasında 0,5 cm&#39;lik kesi yapmak. </li><li> Kalan iki Ekartörleri kullanarak, ön-arka eksen ve mantar pano (Şekil 2B) Retraktörler güvenli olarak toraks açın. </li> &lt;Sol pulmoner arter ve bronş (Şekil 3A, B) maruz kadar sol elinde kavisli künt uçlu forseps kullanarak li&gt; torakotomi ile yanal ve inferior sol akciğer üst kısmını sol akciğer kavramak ve yerinden. </li><li> Avuç aplikatör ve avuç (Şekil 3C) uzak işaret kavisli ucu gövdesi ile sağ elinde yüklü titanyum vasküler mikroklip aplikatör Holding, sol arka yönü eğrilik boyunca toraks içine aplikatör ucu kaydırın Akciğer ve bronşları sol ve pulmoner arter (Şekil 3D) klip. </li><li> Aplikatör çıkarın ama geri sol akciğer tutun. Sağ eli ile künt ucu mikro-makas kavrayın ve klibe bronşları ve pulmoner arter distalinde kesilir ve sol akciğer (Şekil 3E) çıkarın. </li><li> Kaburga Ekartörleri çıkarın. </li><li> İncisi aşağı cilt 1 cm kadar çimdik kavisli künt forseps kullanındeğil, diyafram seviyesinden ve deri yoluyla ve sol göğüs boşluğunda (Şekil 4A, B) 24 G angiocatheter yerleştirin. </li><li> Göğüs boşluğu kapatmak için 4 th yaklaşık iki kesintiye sütür ve 5 inci kaburga yerleştirmek için 5-0 prolen sütür kullanın. </li><li> Cilt Ekartörleri çıkarın. Kesi uzunluğu boyunca cildi yaklaştığı ve cilt kapalı tutkal forseps iki takım kullanın. </li><li> Angiocatheter 3 ml&#39;lik luer-lock şırınga bağlayın ve nazik vakum uygulayarak ve angiocatheter çekerek artık havayı çıkartın. </li><li> Boyun kesi daha önce olduğu gibi forseps iki takım kullanılarak kapalı Tutkal. </li></ol> 5. Fare Sham Pnömonektomi <ol><li> &quot;Fare Pnömonektomi&quot; protokolde belirtildiği gibi sol akciğer Açığa. Sol göğüs boşluğuna hava girmesini sağlamak için kavisli künt forseps ile göğüs kafesini kaldırın (Şekil 5A, B). </li><li> Sol tho içine 24 G angiocatheter yerleştirinSol akciğerin kesmemeye özen yukarıdaki gibi Toraks boşluğu. </li><li> 5-0 prolen sütür kullanarak ve akciğer (Şekil 5C) delinme dikkatli olmak, 3. / 4 th içine dikiş materyali iki uzunlukları ve 5. / 6. kaburga aralar (Şekil 5D) yerleştirin. Sol akciğer herniasyonu risklerini azaltmak için ipe önce dikiş materyali her iki uzunlukları yerleştirin. İki kesintiye dikiş (Şekil 5E) yapmak için sütür materyali bağlayın. </li><li> Torasik kesi üzerindeki deriyi Tutkal, angiocatheter ile artık havayı kaldırmak ve yukarıdaki gibi boyun kesi tutkal. </li></ol> 6. Resüsitasyon, Analjezi ve Kurtarma <ol><li> Izofluran kapatın ve buprenorfın 0.1 mg / kg yönetmek ve serum fizyolojik subkutan 0.5 ml. </li><li> Spontan solunum frekanslarında devam zaman, endotrakeal tüp kaldırmak. </li><li> Tekrar ayaktan kadar fareyi gözlemleyin. Tipik resum YürüyüşEndotrakeal tüp çıkarılmasından sonra birkaç dakika es. </li><li> / N O kurtarmak için bir 27 ° C inkübatör (nemlendirilmiş,% 25 oksijen) fare yerleştirin. NOT: Biz ameliyat sonrası ilk 24 saat için kafes katta su ile ıslatılmış yem birkaç topakları yerleştirin. </li><li> Ameliyat sonrası, günde iki kez, üç gün boyunca intraperitonal enjeksiyon ile buprenorfin, 0.1 mg / kg uygulayın. Hayvanları tutarken cerrahi siteyi açmak için özen gösterin. </li></ol> 7. Fare İzleme <ol><li> Ameliyat sonrası 1, 3, 5 ve 7 gün sonra fareler tartılır. </li></ol>

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The authors have nothing to disclose.

Biz bugüne kadar bildirilen fare PNX ve fare sahte PNX prosedürleri en detaylı açıklamasını sağladı. Biz prosedürü öğrenme araştırmacılar sık ​​karşılaştıkları ortak tuzaklar birkaç okuyucu farkında yaptık, ve biz bu tuzaklar karşısında azaltmak için laboratuvar tarafından geliştirilen çeşitli teknikler belirttiğimiz. Bu modeli kullanan diğer laboratuvarlar diğer bir teknik değişiklikler geliştirilen veya farklı enstrümanlar kullanmak olabilir. Teknikleri farklılıkları de?...

akciğerin başlıca fonksiyonu, bir organizmaya ve atmosfer arasındaki oksijen ve karbon dioksit değişimi sağlamaktır. İnsanlarda, doğumsal ve edinsel koşulları bir dizi bozulmuş akciğer fonksiyonu ile sonuçlanan azalmış akciğer yüzey alanına yol açar. Yani, akciğer - örneğin inhale kortikosteroidler, bronkodilatör, ek oksijen, ve kronik mekanik ventilasyon gibi tedavilerin bir ev sahibi engelli akciğer fonksiyonu 1-3 sonuçlarını hafifletmek için kullanılmasına rağmen, bu koşullar için ideal bir tedavi fonksiyonel akciğer dokusunun yeniden büyümesini teşvik ediyorum yenilenmesi. Memeli doku rejenerasyonu iyi belgelenmiştir. Afrika Dikenli Fare skar oluşumu 4 olmaksızın cildin geniş alanlar yeniden yapabilirsiniz. İnsanlarda distal falanks yaralanma veya ampütasyon 5-7 aşağıdaki yeniden yapabilirsiniz. Aşağıdaki pnömonektomi (PNX), telafi akciğer büyümesi yapmak, 9 fare, sıçan 8 oluşurgs 10, ve 11 insanlarda. Tanım olarak, telafi akciğer büyümesi ilişkili mikrosirkülasyon 12 genişlemesi ile bu genişlemiş hava sahasındaki mevcut hava sahasındaki değil sadece genişleme, ancak yeniden bölümlenmenin içerir. Gen ifadesi analizi bu modeli akciğer gelişimi 13 sinyalizasyon olaylar birçok özetlediği olduğunu göstermiştir. Dört hafta, fare PNX sonra, alveol yüzey alanının ve sahte işlemden geçirilmiş hayvan 14 edilene eşdeğerdir. Bu yazıda, fare pNX ve sahte PNX prosedürlerini açıklar.

<table border="0" cellpadding="0" cellspacing="0" width="1052">
	<tbody>
		<tr height="22">
			<td height="22" style="height:22px;width:263px;">Name of the reagent</td>
			<td style="width:263px;">Company</td>
			<td style="width:263px;">Catalogue number</td>
			<td style="width:263px;">Comments (optional)</td>
		</tr>
		<tr height="101">
			<td height="101" style="height:101px;width:263px;">6-inch Vascular Clip Applicator</td>
			<td style="width:263px;">Teleflex Medical (WECK)</td>
			<td style="width:263px;">137062</td>
			<td style="width:263px;"></td>
		</tr>
		<tr height="101">
			<td height="101" style="height:101px;width:263px;">Horizon Small Titanium Red Clip</td>
			<td style="width:263px;">Teleflex Medical (WECK)</td>
			<td style="width:263px;">1201</td>
			<td style="width:263px;"></td>
		</tr>
		<tr height="121">
			<td height="121" style="height:121px;width:263px;">Narrow Pattern 12cm Curved Forceps</td>
			<td style="width:263px;">Fine Science Tools</td>
			<td style="width:263px;">11003-12</td>
			<td style="width:263px;"></td>
		</tr>
		<tr height="141">
			<td height="141" style="height:141px;width:263px;">Curved Serated 10 cm Graefe Forceps&#160;</td>
			<td style="width:263px;">Fine Science Tools</td>
			<td style="width:263px;">11052-10</td>
			<td style="width:263px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:263px;">Castroviejo Needle Holder</td>
			<td style="width:263px;">Fine Science Tools</td>
			<td style="width:263px;">12565-14</td>
			<td style="width:263px;"></td>
		</tr>
		<tr height="41">
			<td height="41" style="height:41px;width:263px;">Straight 9 cm Strabismus Scissors (Blunt Tip)</td>
			<td style="width:263px;">Fine Science Tools</td>
			<td style="width:263px;">14075-09</td>
			<td style="width:263px;"></td>
		</tr>
		<tr height="41">
			<td height="41" style="height:41px;width:263px;">Straight 8.5 cm Hardened Fine Scissors</td>
			<td style="width:263px;">Fine Science Tools</td>
			<td style="width:263px;">14090-09</td>
			<td style="width:263px;"></td>
		</tr>
		<tr height="41">
			<td height="41" style="height:41px;width:263px;">Straight, Blunt Tip Cohan-Vannas Spring Scissors</td>
			<td style="width:263px;">Fine Science Tools</td>
			<td style="width:263px;">15000-12</td>
			<td style="width:263px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:263px;">Skin Glue</td>
			<td style="width:263px;">Gluture</td>
			<td style="width:263px;">32046</td>
			<td style="width:263px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:263px;">22 ga angiocatheter</td>
			<td style="width:263px;"></td>
			<td style="width:263px;"></td>
			<td style="width:263px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:263px;">24 ga angiocatheter</td>
			<td style="width:263px;"></td>
			<td style="width:263px;"></td>
			<td style="width:263px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:263px;">3 mL luer lock syringe</td>
			<td style="width:263px;"></td>
			<td style="width:263px;"></td>
			<td style="width:263px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:263px;">4 short retractors</td>
			<td style="width:263px;"></td>
			<td style="width:263px;"></td>
			<td style="width:263px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:263px;">2 long retractors</td>
			<td style="width:263px;"></td>
			<td style="width:263px;"></td>
			<td style="width:263px;"></td>
		</tr>
		<tr height="41">
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mouse pneumonectomy model of compensatory lung growth

In humans, disrupted repair and remodeling of injured lung contributes to a host of acute and chronic lung disorders which may ultimately lead to disability or death. Injury-based animal models of lung repair and regeneration are limited by injury-specific responses making it difficult to differentiate changes related to the injury response and injury resolution from changes related to lung repair and lung regeneration. However, use of animal models to identify these repair and regeneration signaling pathways is critical to the development of new therapies aimed at improving pulmonary function following lung injury. The mouse pneumonectomy model utilizes compensatory lung growth to isolate those repair and regeneration signals in order to more clearly define mechanisms of alveolar re-septation. Here, we describe our technique for performing mouse pneumonectomy and sham pneumonectomy. This technique may be utilized in conjunction with lineage tracing or other transgenic mouse models to define molecular and cellular mechanism of lung repair and regeneration.

. Hem PNX ve sahte pnömonektomi için% 100 - pNX ve Sham fare ağırlıkları bir arsa Şekil 6&#39;da verilmiştir Bizim ellerde, hayatta sürekli 95. Sağ akciğer-yetişir yeniden bu model ve beklenen zaman ders, biz Gibney ark. 15 ve Wang ve ark yazmaları okuyucuyu bakın nasıl açıklamaları için. 14 Birkaç ortak tuzaklar başarıyla fare PNX ve fare sahte pnömonektomi prosedürleri gerçekleştirmek için kaçın?...

Watch this Scientific Journal Video about Mouse Pneumonectomy Model of Compensatory Lung Growth at JoVE.com

Mouse Pneumonectomy Model of Compensatory Lung Growth

Mouse pneumonectomy is a commonly employed model of compensatory lung growth. This procedure can be used in conjunction with lineage tracing or transgenic mouse models to elucidate underlying mechanisms.

Telafi Akciğer Büyüme Fare Pnömonektomi Modeli

In humans, disrupted repair and remodeling of injured lung contributes to a host of acute and chronic lung disorders which may ultimately lead to ...

mouse-pneumonectomy-model-of-compensatory-lung-growth

Research

JoVE Journal

Medicine

12.7K Görüntüleme.  Cincinnati Children's Hospital Medical Center. Mouse pneumonectomy is a commonly employed model of compensatory lung growth. This procedure can be used in conjunction with lineage tracing or transgenic mouse models to elucidate underlying mechanisms.

Video: Mouse Pneumonectomy Model of Compensatory Lung Growth

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.

Fare Akciğer Entübasyonun Basit Bir Yöntem

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

Tıp

Diagnostic Ultrasound Imaging of Mouse Diaphragm Function

Function analysis of rodent respiratory skeletal muscles, particularly the diaphragm, is commonly performed by isolating muscle strips using invasive surgical procedures. Although this is an effective method of assessing in vitro diaphragm activity, it involves non-survival surgery. The application of non-invasive ultrasound imaging as an in vivo procedure is beneficial since it not only reduces the number of animals sacrificed, but is also suitable for monitoring disease progression in live mice. Thus, our ultrasound imaging method may likely assist in the development of novel therapies that alleviate muscle injury induced by various respiratory diseases. Particularly, in clinical diagnoses of obstructive lung diseases, ultrasound imaging has the potential to be used in conjunction with other standard tests to detect the early onset of diaphragm muscle fatigue. In the current protocol, we describe how to accurately evaluate diaphragm contractility in a mouse model using a diagnostic ultrasound imaging technique.

Diagnostic ultrasound imaging has proven to be effective in diagnosing various respiratory diseases in human and animal subjects. We demonstrate a comprehensive ultrasound protocol utilized by Dr. Zuo's lab to analyze diaphragm kinetics specifically in mouse models. This is also a non-invasive research technique which can provide quantitative information on mouse respiratory muscle function.

Fare Diyafram Fonksiyonu Diagnostik Ultrason Görüntüleme

Function analysis of rodent respiratory skeletal muscles, particularly the diaphragm, is commonly performed by isolating muscle strips using invasive ...

A Murine Model of Myocardial Ischemia-reperfusion Injury through Ligation of the Left Anterior Descending Artery

Acute or chronic myocardial infarction (MI) are cardiovascular events resulting in high morbidity and mortality. Establishing the pathological mechanisms at work during MI and developing effective therapeutic approaches requires methodology to reproducibly simulate the clinical incidence and reflect the pathophysiological changes associated with MI. Here, we describe a surgical method to induce MI in mouse models that can be used for short-term ischemia-reperfusion (I/R) injury as well as permanent ligation. The major advantage of this method is to facilitate location of the left anterior descending artery (LAD) to allow for accurate ligation of this artery to induce ischemia in the left ventricle of the mouse heart. Accurate positioning of the ligature on the LAD increases reproducibility of infarct size and thus produces more reliable results. Greater precision in placement of the ligature will improve the standard surgical approaches to simulate MI in mice, thus reducing the number of experimental animals necessary for statistically relevant studies and improving our understanding of the mechanisms producing cardiac dysfunction following MI. This mouse model of MI is also useful for the preclinical testing of treatments targeting myocardial damage following MI.

We introduce a surgical method to induce experimental ischemia/reperfusion (I/R) injury to simulate myocardial infarction (MI) in mouse models that allows for more clarity in positioning of the ligation on the left anterior descending artery (LAD) to increase the reproducibility of MI experiments in mice.

Sol ön inen arter ligasyonu ile Miyokard İskemi-reperfüzyon Hasarı bir fare modeli

Acute or chronic myocardial infarction (MI) are cardiovascular events resulting in high morbidity and mortality. Establishing the pathological mechanisms ...

Implantation of Fibrin Gel on Mouse Lung to Study Lung-specific Angiogenesis

Recent significant advances in stem cell research and bioengineering techniques have made great progress in utilizing biomaterials to regenerate and repair damage in simple tissues in the orthopedic and periodontal fields. However, attempts to regenerate the structures and functions of more complex three-dimensional (3D) organs such as lungs have not been very successful because the biological processes of organ regeneration have not been well explored. It is becoming clear that angiogenesis, the formation of new blood vessels, plays key roles in organ regeneration. Newly formed vasculatures not only deliver oxygen, nutrients and various cell components that are required for organ regeneration but also provide instructive signals to the regenerating local tissues. Therefore, to successfully regenerate lungs in an adult, it is necessary to recapitulate the lung-specific microenvironments in which angiogenesis drives regeneration of local lung tissues. Although conventional in vivo angiogenesis assays, such as subcutaneous implantation of extracellular matrix (ECM)-rich hydrogels (e.g., fibrin or collagen gels or Matrigel - ECM protein mixture secreted by Engelbreth-Holm-Swarm mouse sarcoma cells), are extensively utilized to explore the general mechanisms of angiogenesis, lung-specific angiogenesis has not been well characterized because methods for orthotopic implantation of biomaterials in the lung have not been well established. The goal of this protocol is to introduce a unique method to implant fibrin gel on the lung surface of living adult mouse, allowing for the successful recapitulation of host lung-derived angiogenesis inside the gel. This approach enables researchers to explore the mechanisms by which the lung-specific microenvironment controls angiogenesis and alveolar regeneration in both normal and pathological conditions. Since implanted biomaterials release and supply physical and chemical signals to adjacent lung tissues, implantation of these biomaterials on diseased lung can potentially normalize the adjacent diseased tissues, enabling researchers to develop new therapeutic approaches for various types of lung diseases.

Recapitulation of the organ-specific microenvironment, which stimulates local angiogenesis, is indispensable for successful regeneration of damaged tissues. This report demonstrates a novel method to implant fibrin gels on the lung surface of living mouse in order to explore how the lung-specific microenvironment modulates angiogenesis and alveolar regeneration in adult mouse.

Fare Akciğer Fibrin Gel implantasyonu Akciğer özel Anjiogenez Eğitim için

Recent significant advances in stem cell research and bioengineering techniques have made great progress in utilizing biomaterials to regenerate and ...

Method of Isolated Ex Vivo Lung Perfusion in a Rat Model: Lessons Learned from Developing a Rat EVLP Program

The number of acceptable donor lungs available for lung transplantation is severely limited due to poor quality. Ex-Vivo Lung Perfusion (EVLP) has allowed lung transplantation in humans to become more readily available by enabling the ability to assess organs and expand the donor pool. As this technology expands and improves, the ability to potentially evaluate and improve the quality of substandard lungs prior to transplant is a critical need. In order to more rigorously evaluate these approaches, a reproducible animal model needs to be established that would allow for testing of improved techniques and management of the donated lungs as well as to the lung-transplant recipient. In addition, an EVLP animal model of associated pathologies, e.g., ventilation induced lung injury (VILI), would provide a novel method to evaluate treatments for these pathologies. Here, we describe the development of a rat EVLP lung program and refinements to this method that allow for a reproducible model for future expansion. We also describe the application of this EVLP system to model VILI in rat lungs. The goal is to provide the research community with key information and &#8220;pearls of wisdom&#8221;/techniques that arose from trial and error and are critical to establishing an EVLP system that is robust and reproducible.

Method of Isolated Ex Vivo Lung Perfusion in a Rat Model: Lessons Learned from Developing a Rat EVLP Program

Ex-Vivo Lung Perfusion (EVLP) has allowed lung transplantation in humans to become more readily available by enabling the ability to assess organs and expand the donor pool. Here, we describe the development of a rat EVLP program and refinements that allow for a reproducible model for future expansion.

İzole Yöntemi<em&gt; Ex vivo</emBir Rat Modelinde&gt; Akciğer Perfüzyon: Sıçan EVLP Programı Geliştirme Öğrenilmiş Dersler

The number of acceptable donor lungs available for lung transplantation is severely limited due to poor quality. Ex-Vivo Lung Perfusion (EVLP) has allowed ...

Real-time X-ray Imaging of Lung Fluid Volumes in Neonatal Mouse Lung

At birth, the lung undergoes a profound phenotypic switch from secretion to absorption, which allows for adaptation to breathing independently. Promoting and sustaining this phenotype is critically important in normal alveolar growth and gas exchange throughout life. Several in vitro studies have characterized the role of key regulatory proteins, signaling molecules, and steroid hormones that can influence the rate of lung fluid clearance. However, in vivo examinations must be performed to evaluate whether these regulatory factors play important physiological roles in regulating perinatal lung liquid absorption. As such, the utilization of real time X-ray imaging to determine perinatal lung fluid clearance, or pulmonary edema, represents a technological advancement in the field. Herein, we explain and illustrate an approach to assess the rate of alveolar lung fluid clearance and alveolar flooding in C57BL/6 mice at post natal day 10 using X-ray imaging and analysis. Successful implementation of this protocol requires prior approval from institutional animal care and use committees (IACUC), an in vivo small animal X-ray imaging system, and compatible molecular imaging software.

We present a protocol to assess the rate of alveolar fluid clearance or pulmonary edema in neonatal mouse lung using X-ray imaging technology.

Yenidoğan Fare Akciğer Akciğer Akışkan Ciltler Gerçek zamanlı X-ışını görüntüleme

At birth, the lung undergoes a profound phenotypic switch from secretion to absorption, which allows for adaptation to breathing independently. Promoting ...

Apical Resection Mouse Model to Study Early Mammalian Heart Regeneration

Cardiovascular disease plagues the whole world due to intensive lifestyle changes. Heart regeneration holds great promise for repairing and restoring cardiomyocytes lost due to injury and disease. In contrast to the robust cardiac regeneration of certain lower vertebrates, adult mammalian hearts typically show minimal capacity for heart regeneration and repair. However, recent studies have sparked considerable scientific interest with the finding that, between postnatal day 1 to 7 (P1 to P7), the neonatal mouse heart retains significant regenerative potential after apical resection (i.e., surgical amputation and exposure of left ventricular apex). One major controversy over this finding might be due to the diverse surgery-related procedures used in efforts to replicate or expand upon this important finding. These instructions dynamically present the materials and methodology for apical resection in a mouse model. The salient steps of this rodent survival surgery involve hypothermia anesthesia, thoracotomy, surgical amputation of heart ventricular apex, and suture and recovery of mice. The approach described could expand the application of the apical resection mouse model for cardiovascular research.

A step-by-step video protocol of apical resection is demonstrated in this study. Apical resection is a recently highlighted surgical approach in mammalian heart regeneration research. This study may promote the application of apical resection as a standard methodology in research into the mechanism underlying heart regeneration.

Apikal Rezeksiyon Fare Modeli Erken Memeli Kalp Rejenerasyon Eğitim

Cardiovascular disease plagues the whole world due to intensive lifestyle changes. Heart regeneration holds great promise for repairing and restoring ...

Open Tracheostomy Gastric Acid Aspiration Murine Model of Acute Lung Injury Results in Maximal Acute Nonlethal Lung Injury

Acid pneumonitis is a major cause of sterile acute lung injury (ALI) in humans. Acid pneumonitis spans the clinical spectrum from asymptomatic to acute respiratory distress syndrome (ARDS), characterized by neutrophilic alveolitis, and injury to both alveolar epithelium and vascular endothelium. Clinically, ARDS is defined by acute onset of hypoxemia, bilateral patchy pulmonary infiltrates and non-cardiogenic pulmonary edema. Human studies have provided us with valuable information about the physiological and inflammatory changes in the lung caused by ARDS, which has led to various hypotheses about the underling mechanisms. Unfortunately, difficulties determining the etiology of ARDS, as well as a wide range of pathophysiology have resulted in a lack of critical information that could be useful in developing therapeutic strategies.
Translational animal models are valuable when their pathogenesis and pathophysiology accurately reproduce a concept proven in both in vitro and clinical settings. Although large animal models (e.g., sheep) share characteristics of the anatomy of human trachea-bronchial tree, murine models provide a host of other advantages including: low cost; short reproductive cycle lending itself to greater data acquisition; a well understood immunologic system; and a well characterized genome leading to the availability of a variety of gene deletion and transgenic strains. A robust model of low pH induced ARDS requires a murine ALI that targets mainly the alveolar epithelium, secondarily the vascular endothelium, as well as the small airways leading to the alveoli. Furthermore, a reproducible injury with wide differences between different injurious and non-injurious insults is important.
The murine gastric acid aspiration model presented here using hydrochloric acid employs an open tracheostomy and recreates a pathogenic scenario that reproduces the low pH pneumonitis injury in humans. Additionally, this model can be used to examine interaction of a low pH insult with other pulmonary injurious entities (e.g., food particles, pathogenic bacteria).

This protocol induces acute lung injury in a mouse that has close fidelity to the pathogenesis of acid pneumonitis observed in humans. We generate a maximal acute nonlethal low pH lung injury and account for differences in rodent-human anatomic respiratory structure using an open tracheostomy coupled with circumferential pressure release.

Akut Akciğer Hasarı Açık Trakeostomi Gastrik Asit Aspirasyon Fare Modeli Maksimal Akut Ölümcül olmayan Akciğer Hasarı Sonuçlar

Acid pneumonitis is a major cause of sterile acute lung injury (ALI) in humans. Acid pneumonitis spans the clinical spectrum from asymptomatic to acute ...

Integrated Compensatory Responses in a Human Model of Hemorrhage

Hemorrhage is the leading cause of trauma-related deaths, partly because early diagnosis of the severity of blood loss is difficult. Assessment of hemorrhaging patients is difficult because current clinical tools provide measures of vital signs that remain stable during the early stages of bleeding due to compensatory mechanisms. Consequently, there is a need to understand and measure the total integration of mechanisms that compensate for reduced circulating blood volume and how they change during ongoing progressive hemorrhage. The body&#39;s reserve to compensate for reduced circulating blood volume is called the &#39;compensatory reserve&#39;. The compensatory reserve can be accurately evaluated with real-time measurements of changes in the features of the arterial waveform measured with the use of a high-powered computer. Lower Body Negative Pressure (LBNP) has been shown to simulate many of the physiological responses in humans associated with hemorrhage, and is used to study the compensatory response to hemorrhage. The purpose of this study is to demonstrate how compensatory reserve is assessed during progressive reductions in central blood volume with LBNP as a simulation of hemorrhage.

The purpose of this protocol is to demonstrate the techniques for measuring compensatory responses to reduced central blood volume using lower body negative pressure as a noninvasive experimental model of human hemorrhage which can be used to quantify the total integration of compensatory mechanisms to blood volume deficit in humans.

Kanama İnsan Modeli Entegre Telafi Cevapları

Hemorrhage is the leading cause of trauma-related deaths, partly because early diagnosis of the severity of blood loss is difficult. Assessment of ...

Echocardiographic Measurement of Right Ventricular Diastolic Parameters in Mouse

Diastolic dysfunction is a prominent feature of right ventricular (RV) remodeling associated with conditions of pressure overload. However, the RV diastolic function is rarely quantified in experimental studies. This might be due to technical difficulties in the visualization of the RV in the apical four-chamber view in rodents. Here we describe two positions facilitating the visualization of the apical four-chamber view in mice to assess the RV diastolic function.
The apical four-chamber view is enabled by tilting the mouse fixation platform to the left and caudally (LeCa) or to the right and cranially (RiCr). Both positions provide images of comparable quality. The results of the RV diastolic function obtained from two positions are not significantly different. Both positions are comparably easy to perform. This protocol can be incorporated into published protocols and enables detailed investigations of the RV function.

Here we describe and compare two positions for obtaining the apical four-chamber view in mice. These positions enable the quantification of the right ventricular function, provide comparable results, and can be used interchangeably.