Name: A Versatile Mounting Method for Long Term Imaging of Zebrafish Development (Video) | JoVE Journal
Uploaded: 2017-01-26T13:00:00.000+00:00
Duration: 6 min 55 s
Description: Learn a versatile mounting method for long-term live imaging of zebrafish embryos using low melting point agarose. This technique enables free posterior body movement while preserving normal development and cellular dynamics.

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5 minutes

Estelle Hirsinger: Core funding from the Institut Pasteur and Agence Nationale de la Recherche (ANR-10-BLAN-121801 DEVPROCESS). Estelle Hirsinger is from the Centre National de la Recherche Scientifique (CNRS). Benjamin Steventon was funded by the Agence Nationale de la Recherche (ANR- 10-BLAN-121801 DEVPROCESS), then a Roux fellowship (Institut Pasteur) then an AFM-Te&#769;le&#769;thon fellowship (number 16829). He is now supported by a Wellcome Trust/Royal Society Sir Henry Dale Fellowship.

1. Preparation of Solutions and Pulled Glass Needle
<ol>
	<li>Make a 25x stock solution of Tricaine (3-amino benzoic acid ethyl ester, also called ethyl 3-aminobenzoate) at 4 mg/mL in 20 mM Tris pH 8.8 and bring that solution is at pH 7. Aliquot by 4 mL and store at -20 °C. 
	NOTE: The anesthetic Tricaine acts preferentially on neural voltage-gated sodium channels thereby blocking muscle twitching and movement6.</li>
	<li>Make a working solution of Tricaine at a final concentration of 0.17 mg/ml in E3 embryo medium.7 
	NOTE: Make the Tricaine working solution extemporaneously as the pH of this solution drifts.</li>
	<li>Dissolve the low melting point agarose to a final concentration of 1.5% in E3 embryo medium in a 50 mL tube by heating the solution in a microwave. Let this solution equilibrate to 42 - 45 °C in either a water bath or bench-top incubator. If preparing large dishes for vertical light-sheet imaging (step 4), make an additional 25 mL of 1% standard melting agarose in E3 embryo medium.</li>
	<li>Use borosilicate glass with filament capillaries with dimensions of OD 1.20 mm, ID 0.69 mm, length 10 mm.</li>
	<li>If capillaries are pulled on the type of heating-filament needle puller described in the Table of Equipment and Reagents, use the following settings: Heat 600, Pull 120, Velocity 50, Time 225, Pressure 500. With a pair of sharp forceps, break the needle just past the point at which it flexes to create a clean and sharp needle for orientating embryos and removing excess agarose. A micro-scalpel can also be used to remove excess agarose.</li>
</ol>
2. Embedding of Embryos for Inverted or Upright Microscopy
<ol>
	<li>Raise the embryos up to the appropriate stage in E3 embryo medium.7</li>
	<li>At the required stage, dechorionate embryos with a pair of sharp forceps underneath a binocular dissecting microscope.</li>
	<li>Incubate the dechorionated embryos for at least 5 min in the Tricaine working solution.</li>
	<li>Once the melted agarose solution has cooled to 45 °C, use a glass Pasteur pipette to transfer the dechorionated embryo directly into the 50 ml tube with minimal transfer of E3 medium.</li>
	<li>Remove embryo together with approximately 1 ml of mounting medium and add approx. 100 µl of mounting medium together with the embryo to the central circle of a 35 mm glass-bottomed petri dish with a 10 mm microwell.</li>
	<li>As the mounting medium is setting, move the embryo to the edge of the circle of agarose with the tail facing outwards (Figure 1A). Use the capillary needle to maintain the embryo in the desired lateral orientation until the gel is completely set. To image posterior body development, take care to orientate the embryo in as lateral an orientation as possible. Therefore, maintain the embryo in this position by careful adjustments with the capillary needle. 
	NOTE: Multiple embryos can be added to the mounting dish at this point, if required. If this is the case, transfer the low-melt agarose into the dish first and add the embryos to the center of the agarose drop. Then, push the embryos out to the edges of the glass ring and orientate into the desired position. Up to six embryos can be mounted this way before the agarose becomes solidified.</li>
</ol>
3. Removal of Excess Agarose Around the Posterior Body
NOTE: This section describes the procedure by which agarose is removed from the region surrounding the posterior body. In the case of posterior body elongation, it is important to ensure that the tail can grow-out normally. By removing the agarose after the embryo has been completely included by agarose, the embryo is left enclosed by the head region and approximately half of the yolk sac.
<ol>
	<li>Once the agarose drop has set, flood the petri dish with the Tricaine working solution.</li>
	<li>Under a dissecting binocular microscope with a transmitted-light base, adjust the mirror position and angle of incident light such that the strong contrast allows for the cuts in the agarose to be seen clearly through the operation.</li>
	<li>To perform cut 1 (Figure 1), use the capillary needle or the micro-scalpel to cut the agarose mid-way along the yolk, from a position just posterior to the forming heart field to the position of the somite 5 (the 5th anterior somite).</li>
	<li>Start the initial cut adjacent to the forming heart as shown, and the full way through the agarose to the glass.</li>
	<li>Keep the capillary or micro-scalpel deep within the agarose, and slowly saw up and down while beginning to make a long cut over the embryo as shown Figure 1. Cut as close to the embryo as possible without puncturing the embryo or yolk.</li>
	<li>Next, make cuts 2 and 3 (Figure 1), starting from the position against the embryo and with the cut going all the way down to the glass bottomed dish. Make cut 2 so that it is tangential to the first 5 somites, allowing for full dorsalward unfolding of the posterior body. Make cut 3 at a 90° angle with the yolk surface and starting from the heartfield. 
	NOTE: Cutting the agarose until the edge of the glass circle (as shown in Figure 1) aids in removing the agarose as a complete block (step 3.6). However, this is not necessary.</li>
	<li>Starting at the intersection of cuts 1 and 3, make a slow diagonal cut towards the end of cut 2 whilst slowly lifting upwards in order to dislodge the square of agarose surrounding the posterior body. 
	Notes: In some cases, this will be released in one block and the operation is completed in one go. In others, it may take several attempts to dis-lodge all the agarose surrounding the embryo.</li>
	<li>With a pair of sharp forceps, remove the dislodged blocks of agarose from the embryo medium. To aid in this process, move the agarose pieces to the side of the dish and use the wall of the petri dish as support whilst lifting out the agarose pieces.</li>
</ol>
<img alt="Embryo microscopy setup showing agarose embedment, SPIM configuration for optical sectioning." src="/files/ftp_upload/55210/55210fig1.jpg" data-altupdatedat="1788250015000" data-alt="Figure 1"> 
Figure 1: Diagrams of Mounting Set-ups. (A) The diagram shows the position of the mounted embryo within the center glass ring of a petri dish. On the right is a zoom of the embryo with each successive cut through the surrounding agarose shown with dottted red lines. (B) The mounted embryos is diagrammed in lateral view displaying the ease of access for both inverted and upright objectives. (C) A similar digram showing how embryos can be mounted for vertical light sheet imaging set-ups. <a href="http://cloudfront.jove.com/files/ftp_upload/55210/55210fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<ol start="9">
	<li>If muscle twitching is not completely blocked at that point, add drops of Tricaine from the stock solution of 4 mg/ml, pH 7.</li>
</ol>
4. Mounting of Embryos for Vertical Light-sheet Microscopy
NOTE: This is a variation on the method outlined above that allows for the access of multiple objectives for imaging of samples by vertically-orientated SPIM. The idea behind this variation is to lift the sample slightly higher than the bottom of the dish, to allow for easy access of two imaging objectives.
<ol>
	<li>Prior to sample mounting, coat a 100 mm plastic petri dish with 1% agarose in E3 medium to a height of 5 mm and allow to set.</li>
	<li>Place a drop of 1 ml low-melting point agarose to the center of the dish and allow to set.</li>
	<li>Embed embryos in low-melting point agarose as in section 2. However, this time, remove the embryo from the 50 ml tube of agarose with a smaller drop of solution (0.5 ml) and place this small drop on top of the 1 ml drop in the center of the dish.</li>
	<li>Use the capillary needle to place the embryo in the center of the small drop and maintain its correct orientation until gel is set.</li>
	<li>Flood the dish with Tricaine working solution and remove the excess agarose as in section 3 but without cutting through the cushion of 1% standard agarose.</li>
</ol>

<ol><li>Graeden, E., Sive, H. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Live+Imaging+of+the+Zebrafish+Embryonic+Brain+by+Confocal+Microscopy%5BTitle%5D)+AND+%22J+Vis+Exp%22%5BJournal%5D)">Live Imaging of the Zebrafish Embryonic Brain by Confocal Microscopy.</a> J Vis Exp. (26), e1-e2 (2009).</li>
<li>Delaune, E. A., François, P., Shih, N. P., Amacher, S. L. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Single-Cell-Resolution+Imaging+of+the+Impact+of+Notch+Signaling+and+Mitosis+on+Segmentation+Clock+Dynamics%5BTitle%5D)+AND+%22Dev+Cell%22%5BJournal%5D)">Single-Cell-Resolution Imaging of the Impact of Notch Signaling and Mitosis on Segmentation Clock Dynamics.</a> Dev Cell. 23 (5), 995-1005 (2012).</li>
<li>Lawton, A. K., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Regulated+tissue+fluidity+steers+zebrafish+body+elongation%5BTitle%5D)+AND+%22Development%22%5BJournal%5D)">Regulated tissue fluidity steers zebrafish body elongation.</a> Development. 140 (3), 573-582 (2013).</li>
<li>Dray, N., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Cell-Fibronectin+Interactions+Propel+Vertebrate+Trunk+Elongation+via+Tissue+Mechanics%5BTitle%5D)+AND+%22Curr+Biol%22%5BJournal%5D)">Cell-Fibronectin Interactions Propel Vertebrate Trunk Elongation via Tissue Mechanics.</a> Curr Biol. 23 (14), 1335-1341 (2013).</li>
<li>Steventon, B., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Species+tailoured+contribution+of+volumetric+growth+and+tissue+convergence+to+posterior+body+elongation+in+vertebrates%5BTitle%5D)+AND+%22Development%22%5BJournal%5D)">Species tailoured contribution of volumetric growth and tissue convergence to posterior body elongation in vertebrates.</a> Development. 143, 1732-1741 (2016).</li>
<li>Attili, S., Hughes, S. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Anaesthetic+Tricaine+Acts+Preferentially+on+Neural+Voltage-Gated+Sodium+Channels+and+Fails+to+Block+Directly+Evoked+Muscle+Contraction%5BTitle%5D)+AND+%22PLoS+ONE%22%5BJournal%5D)">Anaesthetic Tricaine Acts Preferentially on Neural Voltage-Gated Sodium Channels and Fails to Block Directly Evoked Muscle Contraction.</a> PLoS ONE. 9 (8), 103751-103756 (2014).</li>
<li>Westerfield, M. <a target="_blank" href="https://zfin.org/zf_info/zfbook/zfbk.html">The Zebrafish Book, 5th Edition; A guide for the laboratory use of zebrafish (Danio rerio)</a>. , University of Oregon Press. Eugene. Paperback (2007).</li>
<li>Schröter, C., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Dynamics+of+zebrafish+somitogenesis%5BTitle%5D)+AND+%22Dev+Dyn%22%5BJournal%5D)">Dynamics of zebrafish somitogenesis.</a> Dev Dyn. 237 (3), 545-553 (2008).</li>
<li>Megason, S. G. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((In+toto+imaging+of+embryogenesis+with+confocal+time-lapse+microscopy%5BTitle%5D)+AND+%22Methods+Mol+Biol+%28Clifton%2C+N.J.%29%22%5BJournal%5D)">In toto imaging of embryogenesis with confocal time-lapse microscopy.</a> Methods Mol Biol (Clifton, N.J.). 546, Chapter 19 317-332 (2009).</li>
<li>Sugiyama, M., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Illuminating+cell-cycle+progression+in+the+developing+zebrafish+embryo%5BTitle%5D)+AND+%22PNAS%22%5BJournal%5D)">Illuminating cell-cycle progression in the developing zebrafish embryo.</a> PNAS. 106 (49), 20812-20817 (2009).</li>
</ol>

The authors have nothing to disclose.

This mounting technique enables embryos to be kept still during transfer to the microscope and over long-term time-lapse imaging experiments aimed at following posterior body elongation at multiple length scales. Furthermore, it is versatile in that it allows for imaging on both upright and inverted microscopy set-ups, and a suggestion is made for how this can be further adapted to vertically orientated SPIM.
A critical step in this protocol is the careful removal of excess agarose surrounding...

Posterior body elongation is an essential process in embryonic development by which the embryo extends to form a large part of the body axis. It is an example of a complex morphogenetic process by which multiple cell behaviors act coordinately to generate the morphogenesis at the level of individual tissues. These differential tissue deformations then act together to generate the elongation of the posterior body at the whole structure level. To understand how these processes are controlled and coordinated during development, we must be able to follow these processes at multiple scales (i.e. at the level of molecules, cells, cell populations and tissues) and to relate this directly to the morphogenesis of the entire structure.
Zebrafish embryos are ideal for imaging posterior body elongation as their optical transparency and small size allows for the application of minimally invasive light imaging approaches well suited to live imaging.1 This has been evidenced by a series of recent publications that have shed light on posterior body development at the level of molecules,2 single cells,3 and inter-tissue behaviors,4 as well as at the level of cell population and whole organ.5
Advanced imaging techniques such as confocal, multi-photon microscopy and selective plane illumination microscopy (SPIM) are enabling the long term imaging of developmental processes with decreased effect of light toxicity and photo-bleaching. Robust techniques for the mounting of live samples are required to achieve three goals: 1) sufficient support to maintain samples in the correct orientation during transfer to the microscope and during acquisition, 2) sufficient freedom of movement of the sample to allow for the outgrowth of the posterior body region without affecting its normal development, and finally 3) a certain degree in versatility of the mounting method to allow imaging on diverse imaging set-ups.
This protocol introduces a mounting technique for imaging the development of the zebrafish D. rerio. This technique involves mounting embryos such that the head and yolk sac regions are almost entirely included in agarose, while leaving the posterior body region to elongate and develop normally. As such, it is also an appropriate method for the long-term imaging of other regions of the developing body as the agarose enables imaging by standard light imaging techniques. This protocol demonstrates mounting of embryos in a lateral orientation, although it is also possible to mount embryos in alterative orientations. It will further show how to adapt the method for upright, inverted and vertical light-sheet microscopy setups.

<table><tbody><tr><td>&lt;strong&gt;CONSUMABLES&lt;/strong&gt;</td><td></td><td></td><td></td></tr><tr><td>Glass-bottomed dishes</td><td>Mattek</td><td>P35-1.5-10-C</td><td>35 mm Petri dish, 10 mm microwell. No. 1.5 cover glass</td></tr><tr><td>Capillaries for injection needles</td><td>&amp;nbsp;Sutter&amp;nbsp;</td><td>BF 120-94-10</td><td>We use orosilicate glass with filament, OD 1.20 mm, ID 0.94 mm, length 10 cm. However, filament needles are not necessary and most injection standard needles should work.</td></tr><tr><td>Micro-scalpel</td><td>Feather</td><td>P-715</td><td>Micro Feather disposable opthalmic scalpel with plastic handle</td></tr><tr><td>Pasteur Pipettes</td><td></td><td></td><td>230 mm long</td></tr><tr><td>&lt;strong&gt;REAGENTS&lt;/strong&gt;</td><td></td><td></td><td></td></tr><tr><td>Tricaine</td><td>Sigma-Aldrich</td><td>A5040</td><td></td></tr><tr><td>Low-melting point agarose</td><td>Sigma-Aldrich</td><td>A9414</td><td></td></tr><tr><td>&lt;strong&gt;EQUIPMENT&lt;/strong&gt;</td><td></td><td></td><td></td></tr><tr><td>Fine forceps&amp;nbsp;</td><td>FINE SCIENCE TOOLS GMBH&amp;nbsp;</td><td>11252-30&amp;nbsp;</td><td>Dumont #5</td></tr><tr><td>Needle puller&amp;nbsp;</td><td>Sutter&amp;nbsp;</td><td>P97</td><td>Heating-filament needle puller</td></tr><tr><td>Binocular dissecting microscope</td><td>Leica</td><td>S8 Apo</td><td></td></tr></tbody></table>

a versatile mounting method for long term imaging of zebrafish development

A Versatile Mounting Method for Long Term Imaging of Zebrafish Development

Zebrafish embryos offer an ideal experimental system to study complex morphogenetic processes due to their ease of accessibility and optical transparency. In particular, posterior body elongation is an essential process in embryonic development by which multiple tissue deformations act together to direct the formation of a large part of the body axis. In order to observe this process by long-term time-lapse imaging it is necessary to utilize a mounting technique that allows sufficient support to maintain samples in the correct orientation during transfer to the microscope and acquisition. In addition, the mounting must also provide sufficient freedom of movement for the outgrowth of the posterior body region without affecting its normal development. Finally, there must be a certain degree in versatility of the mounting method to allow imaging on diverse imaging set-ups. Here, we present a mounting technique for imaging the development of posterior body elongation in the zebrafish D. rerio. This technique involves mounting embryos such that the head and yolk sac regions are almost entirely included in agarose, while leaving out the posterior body region to elongate and develop normally. We will show how this can be adapted for upright, inverted and vertical light-sheet microscopy set-ups. While this protocol focuses on mounting embryos for imaging for the posterior body, it could easily be adapted for the live imaging of multiple aspects of zebrafish development.

The protocol outlined above details a versatile technique for the mounting of zebrafish embryos for long-term time lapse imaging. An example of this is shown in Figure 2A and in animated/video Figure 1. Embryos were injected at the 1 cell stage with mRNA encoding the photoconvertible fluorescent protein kikumeGR. At the 15 somite stage they were mounted as described above and imaged for 12 hr on an inverted confocal microscope with a 10X objective. The re...

Here, we present a versatile mounting method that allows for the long-term time-lapse imaging of the posterior body development of live zebrafish embryos without perturbing normal development.

Zebrafish embryos offer an ideal experimental system to study complex morphogenetic processes due to their ease of accessibility and optical transparency. ...

Overall goal of this method is to mount Zebrafish embryos for live imaging, that enables the normal outgrowth of the posterior body region. This method can be adapted for the imaging of other regions of the developing Zebrafish. This technique helps to answer key questions in Developmental Biology, such as how individual cell behaviors lead to the morphogenesis at the level of whole tissues.The main advantage of this technique is that it enables the free moment of the posterior body whilst keeping the embryo in the correct orientation. To begin, add low melting point agarose at a final concentration of 1.5%to E3 medium in a 50 milliliter tube, and dissolve the agarose by heating in the microwave. Allow the solution to equilibrate to 42 to 45 degrees celsius in a water bath or bench top incubator.After pulling glass needles according to the text protocol. With a pair of forceps, break the needle just past the point where it flexes to create a clean and sharp needle for orienting embryos and removing excess agarose. Raise the embryos up to the appropriate stage in E3 medium.Then under a binocular dissecting microscope, use a pair of sharp forceps to dechorionate the embryos. Incubate the dechorionated embryos for at least five minutes in tricaine working solution. Then use a glass Pasteur pipette to transfer the dechorionated embryo with minimal E3 directly into the 50 milliliter tube of 45 degree celsius agarose.Remove the embryo together with approximately one milliliter of the mounting agarose and transfer approximately 100 microliters of the medium with the embryo to the center of a 10 millimeter microwell at the bottom of a 35 millimeter glass bottomed Petri dish. As the mounting medium is setting, move the embryo to the edge of the circle of agarose, with the tail facing outwards. Use the capillary needle to orient the embryo as laterally as possible to image posterior body development.Then with the capillary, maintain the embryo in the desired lateral orientation until the gel is completely set. Once the agarose drop has set, use tricaine working solution to flood the Petri dish. Then, under a dissecting microscope with a transmitted light base, adjust the mirror position and angle of incident light so the strong contrast allows the cuts in the agarose to be clearly seen.To perform cut one, use the capillary needle or micro-scalpel to cut the agarose in a sawing up and down motion, adjacent to and midway along the yolk, just posterior to the forming heart fields down the fifth anterior somite, and completely through the agarose to the glass. Critical here to ensure that the embryo's not damaged while cutting the agarose over the yolk sack. Next, make the second and third cuts, beginning against the embryo down to the glass, tangential to the first five somites, allowing the dorsal unfolding of the posterior body.Then, beginning at the intersection of cuts one and three, make a slow diagonal cut towards the end of cut three while slowly lifting upwards to dislodge the square of agarose surrounding the posterior body. With a pair of sharp forceps, remove the dislodged blocks of agarose from the embryo medium by using the wall of the Petri dish as support while lifting out the agarose pieces. Prior to sample mounting, use 1%agarose in E3 to coat a 100 millimeter plastic dish to a height of five millimeters and allow it to set.Then place a drop of one milliliter low melting point agarose into the center of the dish and allow it to set as well. Embed the embryoes in low melting point agarose as demonstrated earlier in this video. However, this time, remove the embryo from the 50 milliliter tube of agarose with a smaller drop of solution, and place this small drop on top of the one milliliter drop in the center of the dish.Use the capillary needle to position the embryo in the center of the small drop and maintain its correct orientation until the gel is set. Finally, use tricaine working solution to flood the dish and remove the excess agarose. An example of a Zebrafish embryo injected with mRNA encoding for the photoconvertible fluorescent protein kikumeGR, then mounted at the 15 somite stage and subjected to time-lapse imagine for 12 hours is shown in this animated video.The posterior body is allowed to move freely and exhibits similar changes in morphology as seen in embryoes that are allowed to develop free of their chorion in normal culture conditions. In this video, embryoes were injected at the 16 cell stage with mRNA encoding histone 2BRFP, that labels the nuclei, and CAAXGFP, that labels the cell membranes. Images were taken on an upright, multiphoton microscope with a 25X water immersion objective from the 10 somite stage for three hours to visualize cell behaviors during tail bud formation.Cells can be seen generating active protrusions and directional movement as the tail bud forms normally. Once mastered, this technique can be performed in 20 minutes if done properly. While performing this procedure, it is important to make sure that the embryo is in a lateral position while the agarose gel is setting.Otherwise, the region of interest will move rapidly out of the field of view during imaging. After watching this video, you should have a clear understanding of how to mount Zebrafish embryoes for the live imaging of posterior body elongation.

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Learn a versatile mounting method for long-term live imaging of zebrafish embryos using low melting point agarose. This technique enables free posterior body movement while preserving normal development and cellular dynamics.

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