המחברים מבקשים להודות לאורה Lowery אן שפיתח את הטכניקה הזו במעבדה. HS נתמכת על ידי NIHMH70926. ג&#39;ניפר Gutzman נתמך על ידי מענק CSBi / מרק דוקטורט.

פרוטוקול חלק 1: הכנת microinjection <ol style=";text-align:right;direction:rtl"><li style=";text-align:right;direction:rtl"> היכונו הזריקה ידי משיכת מחטים נימי סאטר חולץ באמצעות מכשירים מחט. </li><li style=";text-align:right;direction:rtl"> מלאו את המחט עם פלורסנט לצבוע (כגון טקסס האדום dextran). </li><li style=";text-align:right;direction:rtl"> הר מחט במנגנון micromanipulator ו microinjection. </li><li style=";text-align:right;direction:rtl"> חותכים את המחט לגודל המתאים בזווית כדי ליצור קצה משופעים. </li><li style=";text-align:right;direction:rtl"> מדוד את גודל טיפה ולבדוק כי הוא בין 1-2nl לכל זריקה בשמן. </li></ol> חלק 2: הכנת עוברים <ol style=";text-align:right;direction:rtl"><li style=";text-align:right;direction:rtl"> להזריק את העוברים 30 דקות מוקדם יותר בשלב של עניין. לדוגמה, כדי ללמוד את החדרים ב 24 שעות שלאחר ההפריה (hpf), להזריק את העוברים על hpf 23.5. שלב את העוברים על פי קימל et al. (4). </li><li style=";text-align:right;direction:rtl"> תחת stereomicroscope, בזהירות להסיר את סיסית מן העוברים באמצעות מלקחיים. </li><li style=";text-align:right;direction:rtl"> בעזרת צלחת פלסטיק מצופה agarose 1%, חורים agarose עם טיפ 100-200 פלסטיק פיפטה μl. הסר בזהירות את אטמי agarose מן החורים באמצעות מלקחיים. </li><li style=";text-align:right;direction:rtl"> העברת העוברים בתקשורת העובר לתוך צלחת agarose עם חורים. </li><li style=";text-align:right;direction:rtl"> הוסף tricaine (שנעשו על פי Westerfield (5)) בתקשורת להרדים את העוברים ולמנוע תנועה במהלך הניסוי. </li><li style=";text-align:right;direction:rtl"> בעדינות במקום זנב העובר לתוך החור, לכוון אותו כך מנגנון הזרקת נמצא בצד האחורי של העובר. </li></ol> חלק 3: הזרקת החדר המוח <ol style=";text-align:right;direction:rtl"><li style=";text-align:right;direction:rtl"> כדי להזריק את החדר המוח, לסדר את ההתקנה המיקרומניפולציה כך את קצה המחט באותו שדה הראייה כפי העובר על מתח גבוה. </li><li style=";text-align:right;direction:rtl"> בזהירות את המחט דרך roofplate הדק של למוח האחורי האחורי רק כדי hingepoint r0/r1 בלי לפגוע ברקמת המוח להלן. </li><li style=";text-align:right;direction:rtl"> הזרק מספיק לצבוע לחלוטין למלא את החדרים. זה עלול לקחת כמה זריקות כדי למלא את חלל החדר, תלוי בשלב של העובר. </li></ol> חלק 4: הדמיה <ol style=";text-align:right;direction:rtl"><li style=";text-align:right;direction:rtl"> שימוש נקי של 1% agarose מצופה צלחת, חורים חדשים בצלחת, הסר את המצתים, ולהוסיף tricaine להרדים את העוברים ולמנוע תנועה. </li><li style=";text-align:right;direction:rtl"> מניחים את הזנב של העובר החדר, מוזרק לתוך החור בעמדה עבור תמונה הגבי. </li><li style=";text-align:right;direction:rtl"> קחו את התמונה באמצעות האור המועבר. </li><li style=";text-align:right;direction:rtl"> זה קריטי מאוד שלא להזיז את העובר או מיקרוסקופ. </li><li style=";text-align:right;direction:rtl"> שינוי ההגדרות על המיקרוסקופ לקחת תמונה עם אור ניאון. </li><li style=";text-align:right;direction:rtl"> שנה את מיקום העובר לקחת תמונות לרוחב עם האור הן מועבר אור ניאון. </li><li style=";text-align:right;direction:rtl"> שמור את התמונות כקובצי TIFF עבור עיבוד התמונה Photoshop. </li></ol> חלק 5: עיבוד תמונה <ol style=";text-align:right;direction:rtl"><li style=";text-align:right;direction:rtl"> כדי לעבד את התמונות ב-Photoshop, פתחו את האור המועבר ותמונות אור ניאון של העובר אותו לקח באותה תנוחה. הקפד כל ההגדרות זהים עבור כל תמונה. </li><li style=";text-align:right;direction:rtl"> גרור תמונה פלורסנט שלך על התמונה האור המועבר ולסדר אותן בדיוק. </li><li style=";text-align:right;direction:rtl"> עם התמונה פלורסנט שנבחר, בחר &quot;תמונה&quot;, &quot;התאמות&quot;, ואז &quot;החלף צבע&quot; וגם לשנות את הרקע משחור ללבן. </li><li style=";text-align:right;direction:rtl"> בחלון &quot;החלף צבע&quot; להתאים את גורם &quot;הערפול&quot; ימינה עד התמונות פלורסנט נראה אחיד בצבע. </li><li style=";text-align:right;direction:rtl"> בחלון &quot;שכבות&quot;, בחר &quot;הכפל&quot; להציג את התמונות כיסוי. תמונת חלל החדר שלך צריך להתאים את התמונה בדיוק האור המועבר. </li><li style=";text-align:right;direction:rtl"> שמור את הקובץ וחזור על כל תמונות אחרות. </li></ol> תוצאות נציג / תוצאה פרופר תמונות הזרקת החדר מוצגים באיור 1 לוחות לספירה, ואילו דוגמה תמונות הזרקה שגויה מוצגים EH. זריקות נכונה יש קצוות חדים ולא מפוזר צבע. הזרקה שגויה, אשר מתרחשת כאשר המחט מוחדרת עמוק מדי לתוך החדר והוא פוגע ברקמת המוח להלן, יכול לגרום לצבוע שמחוץ לעין של מרחב החדר ועל החלמון. <img src="/files/ftp_upload/1218/1218figure1.png" alt="איור 1" width="600" height="742" /> באיור 1. החדר זריקות של 25 עוברי hpf סוג בר. (AD) שיטת הזרקה נכונה (EH) שיטת הזרקה שגויה מוצגים כדוגמאות. (A, E) תמונות brightfield הגב עם תמונות פלורסנט המקביל (B, F) את השכבה של תמונות פלורסנט brightfield (C, G) עבור שיטות הזרקת והלא מדויקות המוצג. החצים מצביעים על אזורים בהם לצבוע הלך מעבר בחלל החדר המוח עקב זריקה החדר נכונה (ראה &quot;פתרון בעיות&quot;). Anterior היא שמאלה כל התמונות. פתרון בעיות: <table border="1" style=";text-align:right;direction:rtl"><tbody><tr style="font-weight:bold; font-size:16px;"><td> בעיה </tד&gt; <td> לגרום </td><td> תרופה </td></tr><tr><td> אתה מועך את העובר עם המחט. </td><td> מחט שלך בוטה מדי או טיפ גדול מדי. </td><td> התחל עם מחט חדשה לא לשבור אותו הרחק מאחור. שפוע מחט שלך כדי לעשות את זה חד כמו מחט מזרק. </td></tr><tr><td> הצבע הוא לאורך העובר ואת החלמון (ראה איור 1E-H). </td><td> מחט שלך עבר הרקמה ולא להישאר בחלל החדר. </td><td> מחט שלך עשוי להיות לא חד מספיק, אז אתה לא מצליח לשלוט על מהירות של לנקב. </td></tr><tr><td> צבע הוא חלש מדי או לא forebrain. </td><td> לא להשתמש בלחץ גבוה מספיק עבור הזריקה, או מחט שלך לא היה רחוק מספיק כדי להגיע הקדמי forebrain כאשר הזריקו את צבען. </td><td> להגביר את הלחץ הזרקה או מקום מחט שלך מעט קדמית יותר במהלך הזריקה. אתה יכול לשים את המחט דרך גבול למוח האחורי, המוח התיכון אם ביתר פירוט נדרש forebrain. אתה יכול גם פשוט לחכות קצת בשביל הצבע כדי לפזר עוד לפני הדמיה. </td></tr><tr><td> תמונות פלורסנט שלך חשוך מסביב לקצוות לאחר החלפת צבע Photoshop. </td><td> שכחת לשנות את ההגדרה &quot;הערפול&quot; בחלון להחליף צבע. </td><td> הזיזו את &quot;הערפול&quot; כל הדרך ימינה בחלון להחליף צבע. </td></tr><tr><td> המחט לא לנקב את roofplate למוח האחורי. </td><td> מחט שלך לא נחתך כראוי. </td><td> הפוך את מחט חדשה. אם אתה עושה הרבה זריקות ייתכן שתצטרך מחטים כמה שהם יכולים לקבל משעמם. </td></tr></tbody></table>

<ol>
	<li>Gutzman, J. H. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Formation+of+the+zebrafish+midbrain-hindbrain+boundary+constriction+requires+laminin-dependent+basal+constriction.">Formation of the zebrafish midbrain-hindbrain boundary constriction requires laminin-dependent basal constriction.</a> Mech. Dev. 125, 974-983 (2008).</li><li>Lowery, L. A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Characterization+and+Classification+of+Zebrafish+Brain+Morphology+Mutants.">Characterization and Classification of Zebrafish Brain Morphology Mutants.</a> Anat. Rec. (Hoboken). 292, 94-106 (2009).</li><li>Lowery, L. A., Sive, H. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Initial+formation+of+zebrafish+brain+ventricles+occurs+independently+of+circulation+and+requires+the+nagie+oko+and+snakehead/atp1a1a.1+gene+products.">Initial formation of zebrafish brain ventricles occurs independently of circulation and requires the nagie oko and snakehead/atp1a1a.1 gene products.</a> Development. 132, 2057-2067 (2005).</li><li>Kimmel, C. B. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Stages+of+embryonic+development+of+the+zebrafish.">Stages of embryonic development of the zebrafish.</a> Dev. Dyn. 203, 253-310 (1995).</li><li>Westerfield, M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=.">.</a> The Zebrafish Book: A guide for the laboratory use of zebrafish. , (1995).</li></ol>

בסרטון הזה אנחנו מדגימים איך להזריק צבע פלואורסצנטי (טקסס האדום dextran) לתוך החדרים במוח דג הזברה מתפתח. שיטה זו משמשת כדי להמחיש את המוח בחלל החדר בניגוד neuroepithelium שמסביב שימושי מאוד לקביעת צורה של מרחב החדר, כמו גם את הצורה של רקמת המוח שמסביב. זה מאפשר לנו להבין טוב יות?...

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<html xmlns="http://www.w3.org/1999/xhtml" xml:lang="en" lang="en">	
		
		<div>
		<table border="1">
		<thead>
		<tr>
		<th>Material Name</th>
		<th>Type</th>
		<th>Company</th>
		<th>Catalogue Number</th>
		<th>Comment</th>
		</tr>
		</thead>
		<tbody>
		
<tr>
<td>Forceps</td>
<td>Tool</td>
<td>Fine Science Tools</td>
<td>11252-20</td>
<td>&nbsp;</td>
<tr>
<td>Capillary Tubes (needles)</td>
<td>Tools</td>
<td>Frederick Haer and Co.</td>
<td>30-30-1</td>
<td>&nbsp;</td>
<tr>
<td>Agarose-Coated dishes</td>
<td>Tools</td>
<td>Agarose (Seakem GTG; Lonza) Dishes (Corning) </td>
<td>Agarose (50027) Dishes (430166) </td>
<td>Make agarose approximately 2-3 mm deep in the dish depending on the stage of embryo you are injecting</td>
</tr>
<tr>
<td>Dissecting Microscope</td>
<td>Microscope</td>
<td>Zeiss Stereomicroscope Stemi SV 6 </td>
<td>&nbsp;</td>
<td>&nbsp;</td>
<tr>
<td>Microscope Camera with Fluorescence capabilities and with image capture software</td>
<td>Tools</td>
<td>&nbsp;</td>
<td>&nbsp;</td>
<td>&nbsp;</td>
<tr>
<td>1-200 &mu; pipette tips</td>
<td>Tools</td>
<td>Tip One, US Scientific</td>
<td>1111-0806</td>
<td>These are the perfect size to poke the holes in the agarose and have the embryos fit perfectly.</td>
</tr>
<tr>
<td>Photoshop</td>
<td>Image Analysis</td>
<td>Adobe</td>
<td>&nbsp;</td>
<td>&nbsp;</td>
<tr>
<td>Embryo Loop</td>
<td>Tools</td>
<td>&nbsp;</td>
<td>&nbsp;</td>
<td>Make these yourself with a glass pipette and hair or fishing line and seal with beeswax.</td>
</tr>
<tr>
<td>Microinjector</td>
<td>Tools</td>
<td>Medical Systems Research Products Harvard Apparatus</td>
<td>PL1-100</td>
<td>&nbsp;</td>
<tr>
<td>Needle Puller</td>
<td>Tools</td>
<td>Sutter Instruments</td>
<td>&nbsp;</td>
<td>Settings (Heat 785, Pull 70, Velocity 40, Time 70).</td>
</tr>
<tr>
<td>Micromanipulator</td>
<td>Tools</td>
<td>Narishige</td>
<td>&nbsp;</td>
<td>&nbsp;</td>
<tr>
<td>Fluorescent dye Texas-Red Dextran 70,000MW</td>
<td>Reagent</td>
<td>Molecular Probes</td>
<td>D1830</td>
<td>Other Molecular weights are available if desired.</td>
</tr>
<tr>
<td>Tricaine (3-aminobenzoic acid ethyl ester)</td>
<td>Reagent</td>
<td>Sigma</td>
<td>A-5040</td>
<td>&nbsp;</td>
<tr>
<td>Embryo Media</td>
<td>Reagent</td>
<td>&nbsp;</td>
<td>&nbsp;</td>
<td>According to Westerfield (5)</td>
</tr>		</tbody>
		</table>
		</div>

zebrafish brain ventricle injection

המוח פרופר החדר היווצרות במהלך התפתחות המוח העוברי נדרש תפקוד המוח הנורמלי. חדרי המוח הינם חללים שמור ביותר בתוך המוח, כי הם מלאות בנוזל השדרה. בשנת דג הזברה, לאחר היווצרות בצינור העצבי, neuroepithelium עובר סדרה של המגבלות וקפלי בזמן שהוא מתמלא נוזל וכתוצאה מכך היווצרות החדר המוח. על מנת להבין את תהליך היווצרות החדר, ואת השינויים בצורת neuroepithelial המתרחשות בעת ובעונה אחת, אנחנו צריכים דרך לחזות את החלל החדר לעומת רקמת המוח. עם זאת, טבעו של עוברי דג הזברה שקוף מקשה להבדיל בין רקמות מחלל החדר. לכן, פיתחנו החדר המוח הזרקת טכניקה שבה שטח החדר מתמלא פלורסנט לצבוע הדמיה על ידי brightfield וכן במיקרוסקופ פלואורסצנטי. Brightfield ותמונות פלורסנט מעובדים אז גבי Photoshop. טכניקה זו מאפשרת להדמיה של מרחב החדר עם צבע פלואורסצנטי, בהשוואה בצורת neuroepithelium בתמונה brightfield. החדר המוח הזרקת דג הזברה יכול להיות מועסק מן ההפריה 18 שעות הודעה דרך שלבים מוקדם הזחל. השתמשנו בטכניקה זו בהרחבה, כמו גם באפיון המורפוגנזה מוח מוטציות (1-3) במחקרים שלנו, של היווצרות המוח החדר ואת המורפוגנזה.

Watch this Scientific Journal Video about Zebrafish Brain Ventricle Injection at JoVE.com

Zebrafish Brain Ventricle Injection

לאחר היווצרות בצינור העצבי, neuroepithelium מכווץ קפלי תוך הצינור מתמלא הנוזל השדרתי עובריים (eCSF) כדי ליצור את החדרים במוח העוברי. פיתחנו טכניקה זו זריקה החדר כדי להמחיש טוב יותר את החלל מילא נוזל לעומת הצורה neuroepithelial בעובר חי.

החדר דג הזברה המוח Injection

Proper brain ventricle formation during embryonic brain development is required for normal brain function.  Brain ventricles are the highly conserved ...

Research

JoVE Journal

Biology

21.4K Views.  Whitehead Institute for Biochemical Research. לאחר היווצרות בצינור העצבי, neuroepithelium מכווץ קפלי תוך הצינור מתמלא הנוזל השדרתי עובריים (eCSF) כדי ליצור את החדרים במוח העוברי. פיתחנו טכניקה זו זריקה החדר כדי להמחיש טוב יותר את החלל מילא נוזל לעומת הצורה neuroepithelial בעובר חי.

Video: Zebrafish Brain Ventricle Injection

Live Imaging of the Zebrafish Embryonic Brain by Confocal Microscopy

In this video, we demonstrate the method our lab has developed to analyze the cell shape changes and rearrangements required to bend and fold the developing zebrafish brain (Gutzman et al, 2008). Such analysis affords a new understanding of the underlying cell biology required for development of the 3D structure of the vertebrate brain, and significantly increases our ability to study neural tube morphogenesis. The embryonic zebrafish brain is shaped beginning at 18 hours post fertilization (hpf) as the ventricles within the neuroepithelium inflate. By 24 hpf, the initial steps of neural tube morphogenesis are complete. Using the method described here, embryos at the one cell stage are injected with mRNA encoding membrane-targeted green fluorescent protein (memGFP). After injection and incubation, the embryo, now between 18 and 24 hpf, is mounted, inverted, in agarose and imaged by confocal microscopy. Notably, the zebrafish embryo is transparent making it an ideal system for fluorescent imaging. While our analyses have focused on the midbrain-hindbrain boundary and the hindbrain, this method could be extended for analysis of any region in the zebrafish to a depth of 
80-100 &mu;m.

In this video, we demonstrate a method by which to analyze the developing vertebrate brain in live zebrafish embryos at single cell resolution by confocal microscopy. This includes the method by which we inject the single-cell zebrafish embryo and subsequently mount and image the developing brain.

חיים הדמיה של המוח על ידי עוברי דג הזברה מיקרוסקופיה confocal

In this video, we demonstrate the method our lab has developed to analyze the cell shape changes and rearrangements required to bend and fold the ...

Retro-orbital Injection in Adult Zebrafish

Drug treatment of whole animals is an essential tool in any model system for pharmacological and chemical genetic studies. Intravenous (IV) injection is often the most effective and noninvasive form of delivery of an agent of interest. In the zebrafish (Danio rerio), IV injection of drugs has long been a challenge because of the small vessel diameter. This has also proved a significant hurdle for the injection of cells during hematopoeitic stem cell transplantation. Historically, injections into the bloodstream were done directly through the heart. However, this intra-cardiac procedure has a very high mortality rate as the heart is often punctured during injection leaving the fish prone to infection, massive blood loss or fatal organ damage. Drawing on our experience with the mouse, we have developed a new injection procedure in the zebrafish in which the injection site is behind the eye and into the retro-orbital venous sinus. This retro-orbital (RO) injection technique has been successfully employed in both the injection of drugs in the adult fish as well as transplantation of whole kidney marrow cells. RO injection has a much lower mortality rate than traditional intra-cardiac injection. Fish that are injected retro-orbitally tend to bleed less following injection and are at a much lower risk of injury to a major organ like the heart. Further, when performed properly, injected cells and/or drugs quickly enter the bloodstream allowing compounds to exert their effect on the whole fish and kidney cells to easily home to their niche. Thus, this new injection technique minimizes mortality while allowing efficient delivery of material into the bloodstream of adult fish. Here we exemplify this technique by retro-orbital injection of Tg(globin:GFP) cells into adult casper fish as well as injection of a red fluorescent dye (dextran, Texas Red ) into adult casper fish. We then visualize successful injections by whole animal fluorescence microscopy.

Here we show how to do retro-orbital injection in adult zebrafish.

רטרו מסלולית הזרקה של דג הזברה למבוגרים

Drug treatment of whole animals is an essential tool in any model system for pharmacological and chemical genetic studies. Intravenous (IV) injection is ...

Intraperitoneal Injection into Adult Zebrafish

A convenient method for chemically treating zebrafish is to introduce the reagent into the tank water, where it will be taken up by the fish. However, this method makes it difficult to know how much reagent is absorbed or taken up per fish. Some experimental questions, particularly those related to metabolic studies, may be better addressed by delivering a defined quantity to each fish, based on weight. Here we present a method for intraperitoneal (IP) injection into adult zebrafish. Injection is into the abdominal cavity, posterior to the pelvic girdle. This procedure is adapted from veterinary methods used for larger fish. It is safe, as we have observed zero mortality. Additionally, we have seen bleeding at the injection site in only 5 out of 127 injections, and in each of those cases the bleeding was brief, lasting several seconds, and the quantity of blood lost was small. Success with this procedure requires gentle handling of the fish through several steps including fasting, weighing, anesthetizing, injection, and recovery. Precautions are required to minimize stress throughout the procedure. Our precautions include using a small injection volume and a 35G needle. We use Cortland salt solution as the vehicle, which is osmotically balanced for freshwater fish. Aeration of the gills is maintained during the injection procedure by first bringing the fish into a surgical plane of anesthesia, which allows slow operculum movements, and second, by holding the fish in a trough within a water-saturated sponge during the injection itself. We demonstrate the utility of IP injection by injecting glucose and monitoring the rise in blood glucose level and its subsequent return to normal. As stress is known to increase blood glucose in teleost fish, we compare blood glucose levels in vehicle-injected and non-injected adults and show that the procedure does not cause a significant rise in blood glucose.

We demonstrate intraperitoneal injection into adult zebrafish. We use a 10 &mu;l NanoFil microsyringe controlled by a Micro4 controller and UltraMicroPump III. This demonstration includes the use of cold water as an anesthetic.

הזרקה לתוך intraperitoneal דג הזברה למבוגרים

A convenient method for chemically treating zebrafish is to introduce the reagent into the tank water, where it will be taken up by the fish. However, ...

Direct Delivery of MIF Morpholinos Into the Zebrafish Otocyst by Injection and Electroporation Affects Inner Ear Development

In recent years, electroporation has become a popular technique for in vivo transfection of DNA, RNA, and morpholinos into various tissues, including the eye, brain, and somites of zebrafish. The advantage of electroporation over other methods of genetic manipulation is that specific tissues can be targeted, both spatially and temporally, for the introduction of macromolecules by the application of electrical current. Here we describe the use of electroporation for transfecting mif and mif-like morpholinos into the tissues of the developing inner ear of the zebrafish. In past studies, mif morpholino injected into embryos at the 1- to 8-cell stage resulted in widespread morphological changes in the nervous system and eye, as well as the ear. By targeting the tissues of the inner ear at later stages in development, we can determine the primary effects of MIF in the developing inner ear, as opposed to secondary effects that may result from the influence of other tissues. By using phalloidin and acetylated tubulin staining to study the morphology of neurons, neuronal processes, and hair cells associated with the posterior macula, we were able to assess the efficacy of electroporation as a method for targeted transfection in the zebrafish inner ear. The otic vesicles of 24hpf embryos were injected with morpholinos and electroporated and were then compared to embryos that had received no treatment or had been only injected or electroporated. Embryos that were injected and electroporated showed a decrease in hair cell numbers, decreased innervation by the statoacoustic ganglion (SAG) and fewer SAG neurons compared with control groups. Our results showed that direct delivery of morpholinos into otocysts at later stages avoids the non-specific nervous system and neural crest effects of morpholinos delivered at the 1-8 cell stage. It also allows examination of effects that are directed to the inner ear and not secondary effects on the ear from primary effects on the brain, neural crest or periotic mesenchyme.

A method to deliver morpholinos directly into the zebrafish otocyst at 24hpf has been developed. Using microinjection of morpholinos into the lumen of otic vesicle and electroporation to effect penetration, we were able to bypass the effect of morpholinos on the brain and obtain effects specific to the inner ear.

משלוח ישיר של MIF Morpholinos Into Otocyst דג הזברה על ידי הזרקת electroporation משפיעה על פיתוח האוזן הפנימית

In recent years, electroporation has become a popular technique for in vivo transfection of DNA, RNA, and morpholinos into various tissues, including the ...

In vivo Electroporation of Morpholinos into the Adult Zebrafish Retina

Many devastating inherited eye diseases result in progressive and irreversible blindness because humans cannot regenerate dying or diseased retinal neurons. In contrast, the adult zebrafish retina possesses the robust ability to spontaneously regenerate any neuronal class that is lost in a variety of different retinal damage models, including retinal puncture, chemical ablation, concentrated high temperature, and intense light treatment 1-8. Our lab extensively characterized regeneration of photoreceptors following constant intense light treatment and inner retinal neurons after intravitreal ouabain injection 2, 5, 9. In all cases, resident M&uuml;ller glia re-enter the cell cycle to produce neuronal progenitors, which continue to proliferate and migrate to the proper retinal layer, where they differentiate into the deficient neurons. 
	We characterized five different stages during regeneration of the light-damaged retina that were highlighted by specific cellular responses. We identified several differentially expressed genes at each stage of retinal regeneration by mRNA microarray analysis 10. Many of these genes are also critical for ocular development. To test the role of each candidate gene/protein during retinal regeneration, we needed to develop a method to conditionally limit the expression of a candidate protein only at times during regeneration of the adult retina. 
	Morpholino oligos are widely used to study loss of function of specific proteins during the development of zebrafish, Xenopus, chick, mouse, and tumors in human xenografts 11-14. These modified oligos basepair with complementary RNA sequence to either block the splicing or translation of the target RNA. Morpholinos are stable in the cell and can eliminate or "knockdown" protein expression for three to five days 12. 
	Here, we describe a method to efficiently knockdown target protein expression in the adult zebrafish retina. This method employs lissamine-tagged antisense morpholinos that are injected into the vitreous of the adult zebrafish eye. Using electrode forceps, the morpholino is then electroporated into all the cell types of the dorsal and central retina. Lissamine provides the charge on the morpholino for electroporation and can be visualized to assess the presence of the morpholino in the retinal cells. 
	Conditional knockdown in the retina can be used to examine the role of specific proteins at different times during regeneration. Additionally, this approach can be used to study the role of specific proteins in the undamaged retina, in such processes as visual transduction and visual processing in second order neurons.

In vivo Electroporation of Morpholinos into the Adult Zebrafish Retina

A method to conditionally knockdown a target protein&#x2019;s expression in the adult zebrafish retina is described, which involves intravitreally injecting antisense morpholinos and electroporating them into the retina. The resulting protein is knocked down for several days, which allows testing the protein&#x2019;s role in the regenerating or intact retina.

ב electroporation vivo של Morpholinos לתוך הרשתית דג הזברה למבוגרים

Many devastating inherited eye diseases result in progressive and irreversible blindness because humans cannot regenerate dying or diseased retinal ...

In vivo Electroporation of Morpholinos into the Regenerating Adult Zebrafish Tail Fin

Certain species of urodeles and teleost fish can regenerate their tissues. Zebrafish have become a widely used model to study the spontaneous regeneration of adult tissues, such as the heart1, retina2, spinal cord3, optic nerve4, sensory hair cells5, and fins6.
The zebrafish fin is a relatively simple appendage that is easily manipulated to study multiple stages in epimorphic regeneration. Classically, fin regeneration was characterized by three distinct stages: wound healing, blastema formation, and fin outgrowth. After amputating part of the fin, the surrounding epithelium proliferates and migrates over the wound. At 33 &deg;C, this process occurs within six hours post-amputation (hpa, Figure 1B)6,7. Next, underlying cells from different lineages (ex. bone, blood, glia, fibroblast) re-enter the cell cycle to form a proliferative blastema, while the overlying epidermis continues to proliferate (Figure 1D)8. Outgrowth occurs as cells proximal to the blastema re-differentiate into their respective lineages to form new tissue (Figure 1E)8. Depending on the level of the amputation, full regeneration is completed in a week to a month.
The expression of a large number of gene families, including wnt, hox, fgf, msx, retinoic acid, shh, notch, bmp, and activin-betaA genes, is up-regulated during specific stages of fin regeneration9-16. However, the roles of these genes and their encoded proteins during regeneration have been difficult to assess, unless a specific inhibitor for the protein exists13, a temperature-sensitive mutant exists or a transgenic animal (either overexpressing the wild-type protein or a dominant-negative protein) was generated7,12. We developed a reverse genetic technique to quickly and easily test the function of any gene during fin regeneration.
Morpholino oligonucleotides are widely used to study loss of specific proteins during zebrafish, Xenopus, chick, and mouse development17-19. Morpholinos basepair with a complementary RNA sequence to either block pre-mRNA splicing or mRNA translation. We describe a method to efficiently introduce fluorescein-tagged antisense morpholinos into regenerating zebrafish fins to knockdown expression of the target protein. The morpholino is micro-injected into each blastema of the regenerating zebrafish tail fin and electroporated into the surrounding cells. Fluorescein provides the charge to electroporate the morpholino and to visualize the morpholino in the fin tissue.
This protocol permits conditional protein knockdown to examine the role of specific proteins during regenerative fin outgrowth. In the Discussion, we describe how this approach can be adapted to study the role of specific proteins during wound healing or blastema formation, as well as a potential marker of cell migration during blastema formation.

In vivo Electroporation of Morpholinos into the Regenerating Adult Zebrafish Tail Fin

We describe a method to conditionally knockdown the expression of a target protein during adult zebrafish fin regeneration. This technique involves micro-injecting and electroporating antisense oligonucleotide morpholinos into fin tissue, which allows testing the protein&#x2019;s role in various stages of fin regeneration, including wound healing, blastema formation, and regenerative outgrowth.

ב electroporation vivo של Morpholinos לתוך למבוגרים התחדשות זנב סנפיר דג הזברה

Certain species of urodeles and teleost fish can regenerate their tissues. Zebrafish have become a widely used model to study the spontaneous regeneration ...

Microgavage of Zebrafish Larvae

The zebrafish has emerged as a powerful model organism for studying intestinal development1-5, physiology6-11, disease12-16, and host-microbe interactions17-25. Experimental approaches for studying intestinal biology often require the in vivo introduction of selected materials into the lumen of the intestine. In the larval zebrafish model, this is typically accomplished by immersing fish in a solution of the selected material, or by injection through the abdominal wall. Using the immersion method, it is difficult to accurately monitor or control the route or timing of material delivery to the intestine. For this reason, immersion exposure can cause unintended toxicity and other effects on extraintestinal tissues, limiting the potential range of material amounts that can be delivered into the intestine. Also, the amount of material ingested during immersion exposure can vary significantly between individual larvae26. Although these problems are not encountered during direct injection through the abdominal wall, proper injection is difficult and causes tissue damage which could influence experimental results. We introduce a method for microgavage of zebrafish larvae. The goal of this method is to provide a safe, effective, and consistent way to deliver material directly to the lumen of the anterior intestine in larval zebrafish with controlled timing. Microgavage utilizes standard embryo microinjection and stereomicroscopy equipment common to most laboratories that perform zebrafish research. Once fish are properly positioned in methylcellulose, gavage can be performed quickly at a rate of approximately 7-10 fish/ min, and post-gavage survival approaches 100% depending on the gavaged material. We also show that microgavage can permit loading of the intestinal lumen with high concentrations of materials that are lethal to fish when exposed by immersion. To demonstrate the utility of this method, we present a fluorescent dextran microgavage assay that can be used to quantify transit from the intestinal lumen to extraintestinal spaces. This test can be used to verify proper execution of the microgavage procedure, and also provides a novel zebrafish assay to examine intestinal epithelial barrier integrity under different experimental conditions (e.g. genetic manipulation, drug treatment, or exposure to environmental factors). Furthermore, we show how gavage can be used to evaluate intestinal motility by gavaging fluorescent microspheres and monitoring their subsequent transit. Microgavage can be applied to deliver diverse materials such as live microorganisms, secreted microbial factors/toxins, pharmacological agents, and physiological probes. With these capabilities, the larval zebrafish microgavage method has the potential to enhance a broad range of research fields using the zebrafish model system.

We present a novel method for microgavage of larval zebrafish utilizing standard embryo microinjection and stereomicroscopy equipment. We demonstrate that microgavage is a safe and efficient technique useful for delivering controlled amounts of diverse materials specifically into the larval zebrafish intestinal lumen.

Microgavage של זחלי דג זברה

The zebrafish has emerged as a powerful model organism for studying intestinal development1-5, physiology6-11, disease12-16, and host-microbe ...

Gavaging Adult Zebrafish

The zebrafish has become an important in vivo model in biomedical research. Effective methods must be developed and utilized to deliver compounds or agents in solutions for scientific research. Current methods for administering compounds orally to adult zebrafish are inaccurate due to variability in voluntary consumption by the fish. A gavage procedure was developed to deliver precise quantities of infectious agents to zebrafish for study in biomedical research. Adult zebrafish over 6 months of age were anesthetized with 150 mg/L of buffered MS-222 and gavaged with 5 &mu;l of solution using flexible catheter implantation tubing attached to a cut 22-G needle tip. The flexible tubing was lowered into the oral cavity of the zebrafish until the tip of the tubing extended past the gills (approximately 1 cm). The solution was then injected slowly into the intestinal tract. This method was effective 88% of the time, with fish recovering uneventfully. This procedure is also efficient as one person can gavage 20-30 fish in one hour. This method can be used to precisely administer agents for infectious diseases studies, or studies of other compounds in adult zebrafish.

The increasing use of zebrafish as an animal model requires the development of effective methods for the delivery of known quantities of compounds and solutions. The gavage procedure described below allows for the oral delivery of precise volumes of solution reliably, safely and efficiently to adult zebrafish.

Gavaging דג הזברה למבוגר

The zebrafish has become an important in vivo model in biomedical research. Effective methods must be developed and utilized to deliver compounds or ...

Reverse Genetic Morpholino Approach Using Cardiac Ventricular Injection to Transfect Multiple Difficult-to-target Tissues in the Zebrafish Larva

The zebrafish is an important model to understand the cell and molecular biology of organ and appendage regeneration. However, molecular strategies to employ reverse genetics have not yet been adequately developed to assess gene function in regeneration or tissue homeostasis during larval stages after zebrafish embryogenesis, and several tissues within the zebrafish larva are difficult to target. Intraventricular injections of gene-specific morpholinos offer an alternative method for the current inability to genomically target zebrafish genes in a temporally controlled manner at these stages. This method allows for complete dispersion and subsequent incorporation of the morpholino into various tissues throughout the body, including structures that were formerly impossible to reach such as those in the larval caudal fin, a structure often used to noninvasively research tissue regeneration. Several genes activated during larval finfold regeneration are also present in regenerating adult vertebrate tissues, so the larva is a useful model to understand regeneration in adults. This morpholino dispersion method allows for the quick and easy identification of genes required for the regeneration of larval tissues as well as other physiological phenomena regulating tissue homeostasis after embryogenesis. Therefore, this delivery method provides a currently needed strategy for temporal control to the evaluation of gene function after embryogenesis.&#160;

An adaptable reverse genetic method for zebrafish to assess gene function during later stages of development and physiological homeostasis such as tissue regeneration using intraventricular injections of gene-specific morpholinos.

הפוך גישת morpholino גנטית באמצעות הזרקת לב חדרית לtransfect רקמות קשה ליעד מרובים בזחל דג הזברה

The zebrafish is an important model to understand the cell and molecular biology of organ and appendage regeneration. However, molecular strategies to ...

Nephrotoxin Microinjection in Zebrafish to Model Acute Kidney Injury

The kidneys are susceptible to harm from exposure to chemicals they filter from the bloodstream. This can lead to organ injury associated with a rapid decline in renal function and development of the clinical syndrome known as acute kidney injury (AKI). Pharmacological agents used to treat medical circumstances ranging from bacterial infection to cancer, when administered individually or in combination with other drugs, can initiate AKI. Zebrafish are a useful animal model to study the chemical effects on renal function in vivo, as they form an embryonic kidney comprised of nephron functional units that are conserved with higher vertebrates, including humans. Further, zebrafish can be utilized to perform genetic and chemical screens, which provide opportunities to elucidate the cellular and molecular facets of AKI and develop therapeutic strategies such as the identification of nephroprotective molecules. Here, we demonstrate how microinjection into the zebrafish embryo can be utilized as a paradigm for nephrotoxin studies.

Renal injuries incurred from nephrotoxins, which include drugs ranging from antibiotics to chemotherapeutics, can result in complex disorders whose pathogenesis remains incompletely understood. This protocol demonstrates how zebrafish can be used for disease modeling of these conditions, which can be applied to the identification of renoprotective measures.

Nephrotoxin Microinjection דג הזברה למודל אי-ספיקת כליות חריפה

The kidneys are susceptible to harm from exposure to chemicals they filter from the bloodstream. This can lead to organ injury associated with a rapid ...