The establishment of the presented research model was supported by KMU-innovativ (FKZ: 13GW0037F) of the Federal Ministry of Education and Research Germany.

This protocol follows the ethical guidelines of our institution. In accordance with the statutes of our institution&#39;s ethical review committee no ethical approval had to be obtained prior to the experiments, as all porcine corneas were obtained from the local slaughterhouse.
1. Organ culture
<ol>
	<li>Prepare pig eyes.
	<ol>
		<li>From the local slaughterhouse, obtain pig eyes that were removed shortly postmortem but before thermal treatment. Transport the eyes to the lab and process them within a few hours. During transport, keep the eyes at room temperature (approximately 21 &#176;C) before processing.</li>
		<li>Remove all orbital adnexes (eye muscles, conjunctiva, adipose tissue) prior to disinfection using eye scissors and colibri forceps. Separate and discard all eyes with obvious trauma, external damage (e.g., knife cut), or visible corneal opacities.</li>
		<li>Prepare a 5% iodine-PBS-solution (1:20) in a sterile cup by adding 3 mL of 7.5% povidone iodine to 57 mL of a phosphate buffered saline (PBS) solution. Also prepare a separate sterile cup containing 60 mL pure PBS. 
		NOTE: The total amount of used iodine-PBS-solution and the size of the cup depends on the number of corneas to be dissected. Five to six eyes require approximately 60 mL of the 5%-iodine-PBS-solution to be disinfected properly.</li>
		<li>Put five to six eyes into the 5%-iodine-PBS solution for a total of 5 min to properly disinfect the eyes&#39; surface. Carefully stir every minute to ensure the eyes&#39; surface is fully submerged and disinfected completely in the iodine solution.</li>
		<li>After 5 min, transfer the disinfected eyes to the prepared cup filled with pure PBS. Again, carefully stir to ensure the iodine-PBS-solution is washed away from the eyes&#39; surface. 
		NOTE: Perform this step on a clean bench to prevent contamination of the disinfected eyes.</li>
	</ol>
	</li>
	<li>Prepare cell culture plates. 
	NOTE: Perform the following steps on a clean bench with constant laminar air flow.
	<ol>
		<li>Thaw 2 mL of fetal calf serum (FCS). Fill a syringe (5 mL) with the FCS using a blunt cannula. Empty the syringe through a syringe filter (0.22 &#181;m) to prevent possible bacterial contaminationof the FCS into 80 mL of dextran-free culture medium I (minimum essential medium [MEM] with Earle&#39;s salts, penicillin/streptomycin, L-glutamine [200 mM], amphotericin B [250 &#181;g/mL], Hepes buffer [1 M] [50x], NaHCO3, and distilled water). Agitate the mixture to ensure even substrate distribution.</li>
		<li>Fill each well of a 12 well cell culture plate with 3 mL of the substrate mixture.</li>
	</ol>
	</li>
	<li>Perform dissection and incubation. 
	NOTE: Perform this step on a clean bench. Do not touch the corneal endothelium with any instruments.
	<ol>
		<li>Transfer an eye bulb from the cup with PBS into the eye bulb holder with the cornea facing up and place it beneath an ophthalmic surgical microscope. Use a syringe filled with 0.9% NaCl to slightly apply some suction to the eye over the eye bulb holder to fixate the eye in position for dissection.</li>
		<li>Use a trephine (&#248; 7.5 mm) containing a standardized inlay, which ensures the trephined depth will not exceed 300 &#181;m, to cut superficially into the central cornea (Figure 1A).</li>
		<li>Use colibri forceps and a single-use scalpel with a triangular blade to cut and remove the partially trephined part of the cornea horizontally through the stroma. Discard the separated corneal part consisting of the corneal epithelium, the bowman layer, and a part of the stroma. 
		NOTE: Strictly maintain the horizontal cutting direction to obtain an even thickness of the remaining stroma.</li>
		<li>Superficially place a 10-0 suture (10-0 polyamide 6) into the stroma to be able to differentiate the endothelial from the stromal side during the experiments (Figure 1B). Prevent penetration of the corneal endothelium. Discard the eye bulb if the endothelium is penetrated. 
		NOTE: Penetration of the corneal endothelium with the suturing needle will be visible, as fluid from the anterior eye chamber will leak through the suture channel.</li>
		<li>Use the trephine without the inlay to advance the trephined cut to full depth until the anterior eye chamber is reached (Figure 1C). A distinct drop in resistance and fluid leaking from the anterior eye chamber can be perceived after complete penetration of the cornea. 
		NOTE: Use a hockey knife if the split corneal button remains attached on one side of the split corneal button after trephination.</li>
		<li>Transfer the obtained split corneal button, now consisting of a part of the stroma (Figure 2), the Descemet&#39;s membrane, and the corneal endothelium, into the culture medium (culture medium I + FCS, see section 1.2) into the 12 well cell culture plate with the tagged side facing down, so that the corneal endothelium is facing up. 
		NOTE: If the endothelial side is facing down, the endothelium may get damaged.</li>
		<li>Assign an individual number to every split corneal button for identification during the follow ups and label the wells on the cell culture plate accordingly.</li>
		<li>Incubate the filled cell culture plates in an incubator under standard conditions at a temperature of 37 &#176;C, 5% CO2 and a relative air moisture of 95%. Change the culture medium (culture medium I + FCS) on day 8 if an incubation period of 7 days is exceeded. 
		NOTE: The incubation procedure using split corneal buttons has been validated for up to 15 days.</li>
	</ol>
	</li>
</ol>
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/60171/60171fig1.jpg" /> 
Figure 1: Dissection of the porcine cornea to obtain split corneal buttons. (A) After trephination of the cornea using a trephine with an inlay to cut into a depth of 300 &#181;m and removal of the epithelium and parts of the stromal tissue, (B) a suture is placed superficially into the stroma without penetration of the corneal endothelium for later identification of the stromal side. (C) Full trephination of the remaining cornea is followed by (D) the removal of the obtained split corneal button from the eye bulb. <a href="https://www.jove.com/files/ftp_upload/60171/60171fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
2. Microscopy and examination of the endothelium
<ol>
	<li>Perform unstained examination. 
	NOTE: Unstained examination can be performed multiple times (e.g., at weekly follow ups on day 1, 8, and 15). However, unstained counting only allows the assessment of endothelial cell density, not morphological parameters.
	<ol>
		<li>Fill 3 mL of hypotonic balanced salt solution (hBSS, see composition in Table of Materials) in each well of a 12 well cell culture plate. Carefully place a single split corneal button in hBSS to induce swelling of the corneal endothelial cells and improve visibility of the cells for cell counting. 
		NOTE: Make sure that the endothelial side is facing the direction of the microscope. If an inverted phase contrast microscope is used, the endothelial side needs to be facing downwards. While in place, the culture plate should not be moved to prevent endothelial cell damage.</li>
		<li>Let the cells swell for 1-2 min before taking a picture of the endothelium with the camera attached to the microscope. Take at least three photographs of at least three different areas in order to obtain a representative impression of the actual condition of the corneal endothelium. Add a scale bar with the true to scale length of 100 &#181;m for later analysis of the corneal endothelial cell density and morphological parameters.</li>
		<li>To prevent osmotic damage, remove the split corneal button from the hBSS after a maximum of 5 min and transfer it back into the culture medium3.</li>
	</ol>
	</li>
	<li>Perform stained examination. 
	NOTE: Staining terminates the experiments, as the staining substances used are cytotoxic. Therefore, staining may only be performed at the end of the observation period for the assessment of morphological parameters (reformation figures, rosette formations, alizarin red stained cells).
	<ol>
		<li>Prepare a 0.25% trypan blue solution and 0.2% alizarin red S solution for the staining procedure.
		<ol>
			<li>For the 0.25% trypan blue solution, dilute the 0.4% trypan blue solution with a 0.9% NaCl solution. 
			NOTE: For example, to obtain 20 mL of a 0.25% trypan blue solution, dilute 12.5 mL of the 0.4% trypan blue solution with 7.5 mL of the 0.9% NaCl solution. The trypan blue solution may be stored at room temperature for several weeks or months.</li>
			<li>To obtain a 0.2% alizarin red S solution dissolve 100 mg of the alizarin red S powder in 50 mL of a 0.9% NaCl solution under constant stirring and heating to 50 &#176;C on a magnet stirring plate with heating function. To remove possible precipitates, filter the obtained solution. Adjust the pH of alizarin red S solution to pH 4.2 by adding sodium hydroxide or hydrochloric acid accordingly. 
			NOTE: Before each application of the alizarin red S solution make sure the pH is corrected to 4.2 and that there are no precipitates in the solution. The solution may be stored at room temperature. Do not store the solution for longer than 4 weeks.</li>
		</ol>
		</li>
		<li>Place the split corneal buttons in Petri dishes with the endothelial side facing upwards in order to stain the endothelial cells. Use a pipette to slowly drip the 0.25% trypan blue solution drop by drop onto the corneal endothelium for 90 s. 
		NOTE: Trypan blue allows identification of damaged corneal cells with a permeable membrane because it stains their nuclei.</li>
		<li>Carefully rinse the split corneal button 3x in 0.9% NaCl in a small glass beaker. Again, use a pipette to slowly drip the 0.2% alizarin red S solution drop by drop onto the corneal endothelium for 90 s. 
		NOTE: Alizarin red S stains the Descemet&#39;s membrane, which helps to highlight cell borders in undamaged corneal endothelial cells and to highlight destroyed cells when the underlying Descemet&#39;s membrane becomes visible. Also, it enables easy identification of larger destroyed areas.</li>
		<li>For examination of the stained corneal endothelium follow the steps explained for unstained counting in section 2.1.</li>
	</ol>
	</li>
</ol>
3. Analysis of the corneal endothelial cell density and morphological parameters
<ol>
	<li>Project counting squares on the pictures using a graphics editing software (Table of Materials).
	<ol>
		<li>Open the software and open an image of the corneal endothelium by selecting File | Open | Select.</li>
		<li>Project a square with a true to scale side length of 100 &#181;m on the image. 
		NOTE: The following steps of section 3.1.2 can be ignored if the viewing software allows for the projecting of counting squares onto the picture. The side length of the square depends on the resolution of the images taken with the microscope&#39;s camera and can be calculated with the scale bar.
		<ol>
			<li>Crop the scale bar from the photograph taken with the microscope: select the Rectangular Marquee Tool on the tool bar or press M, then border the scale bar, then select Edit | Crop or press Ctrl + X.</li>
			<li>Click File | New (or press Ctrl + N). On the upcoming window select Clipboard in the Document Type drop-down list. The number of pixels shown is the side length of the counting square. Note the corresponding pixels for the other pictures and click OK.</li>
			<li>Select File | New (or Ctrl + N). Insert width and length (in pixels) of the counting square in the upcoming window according to the length of the scale bar. Select background color White, then press OK.</li>
			<li>Click Select | Select all (or Ctrl + A). Select Edit | Copy (or Ctrl + C).</li>
			<li>Select the image of the corneal endothelium opened in step 3.1.1. Select Edit | Paste (or Ctrl + V) to insert the square on the photo of the corneal endothelium.</li>
			<li>Select the square&#39;s layer and adjust the transparency. Select Layer | Layer Style | Blending Options | Set Opacity to 30% | OK.</li>
			<li>Save the image with the projected square with a true to scale side length of 100 &#181;m. Repeat with the other pictures needed for analysis.</li>
		</ol>
		</li>
	</ol>
	</li>
	<li>Assess the endothelial cell density and morphological parameters.
	<ol>
		<li>Open the images with the projected squares in ImageJ (Version 1.50i) and use the CellCounter PlugIn to count the cells within the square. Open ImageJ, select File | Open (or Ctrl + O) | Select Image. 
		NOTE: ImageJ and the CellCounter PlugIn are freeware available for download online.</li>
		<li>Select Plugins | Cell_Counter | Cell Counter | Initialize. Count the endothelial cells and record the result. On two sides of the square, count the cells that are cut by the square&#39;s edge. Do not count cut cells on the other two sides.</li>
		<li>Analyze at least six squares per cornea from different areas (e.g., three pictures, two squares per picture) and determine the average corneal endothelial cell density per square (100 &#181;m2). Extrapolate the endothelial cell density per 100 &#181;m2 to 1 mm2 by multiplying by 100.</li>
	</ol>
	</li>
	<li>For the assessment of morphological changes, count reformation figures (joint meeting of &#8805;4 cells/cell borders instead of three), rosette formations (characteristic rosette-shaped appearance, five or more radially arranged cells surrounding a destroyed cell), or alizarin red areas (destroyed cells) in the projected squares. 
	NOTE: Alternatively, it may be useful to use larger squares (e.g., 200 x 200 &#181;m2) for morphological analysis in well-preserved samples to obtain more representative results.</li>
</ol>

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The authors have nothing to disclose.

This protocol provides a method for the preparation of porcine split corneal buttons, which represents a standardized and low-cost ex vivo corneal endothelial organ culture model for research purposes6. Porcine split corneal buttons showed a decrease of the endothelial cell density comparable to endothelial cell losses observed in human donor corneas cultivated in eye banks over a two-week period6,10,11<s...

Corneal transplantation procedures are among the most commonly performed transplantations worldwide1. As there is a severe shortage of human donor corneas, experimental research addressing corneal endothelial cells in human corneas is difficult to perform1. However, the introduction of irrigation solutions and other substances used within the eye, ophthalmic viscoelastic devices, as well as surgical instruments and techniques (e.g., phacoemulsification instruments and techniques, ultrasound energy) requires valid and extensive investigations regarding their effects on the corneal endothelium before clinical use.
Few alternatives to human donor corneas exist for research. Animal research models are very valuable but at the same time very resource consuming and increasingly questioned ethically. A major drawback of in vitro cell cultures is their limited translation to the human eye. Results obtained from cell cultures can be incongruous to in vivo conditions, because cells may undergo endothelial mesenchymal transition (EMT), resulting in fibroblast-like morphology caused by the loss of cell polarity and changes in cell shape and gene expression2.
Whereas previous ex vivo models reported cultivation periods of up to only 120 h, a novel preparation technique to establish a porcine corneal endothelial organ culture model by culturing fresh pig corneas for at least 15 days was recently introduced3,4,5,6. If the corneal epithelium and parts of the stroma are removed (approximately 300 &#181;m in total) from the cornea prior to cultivation, swelling of the stroma is reduced in split corneal buttons resulting in less endothelial cell loss and a well maintained endothelial cell layer after up to 15 days, whereas non-split corneal buttons show significant endothelial cell loss due to uneven stromal swelling and formation of Descemet's folds. Eye banks usually use osmotic deswelling agents such as dextran to reduce swelling of corneas prior to transplantation. However, these agents were shown to induce increased endothelial cell loss7,8,9.
This article aims to visualize this standardized ex vivo research model in a detailed step-by-step protocol in order to enable future investigators to perform research on the corneal endothelium using split corneal buttons. This model represents a straightforward method to test substances and techniques used within the eye, such as ophthalmic viscoelastic devices, irrigation solutions, and ultrasound energy, or other procedures where the corneal endothelium is of interest.

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Subject</td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Pig eyes</td>
			<td>local abbatoir</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Substances</td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Alizarin red S</td>
			<td>Sigma-Aldrich, USA</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Culture Medium 1, #F9016</td>
			<td>Biochrom GmbH, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Dulbecco&#39;s PBS (1x)</td>
			<td>Gibco, USA</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Fetal calf serum</td>
			<td>Biochrom GmbH, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Hydrochloric acid (HCl) solution</td>
			<td>own production</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Hypotonic balanced salt solution</td>
			<td>own production</td>
			<td></td>
			<td>per 1 L of H2O: NaCl 4.9 g; KCl 0.75 g; CaCl x H2O 0.49 g; MgCl2 x H2O 0.3 g; Sodium Acetate x 3 H2O 3.9 g; Sodium Citrate x 2 H2O 1.7 g</td>
		</tr>
		<tr>
			<td>Povidon iodine 7.5%, Braunol</td>
			<td>B. Braun Melsungen AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Sodium chloride (NaCl) 0.9%</td>
			<td>B. Braun Melsungen AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Sodium hydroxide (NaOH) solution</td>
			<td>own production</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Trypan blue 0.4%</td>
			<td>Sigma-Aldrich, USA</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Materials &#38; Instruments</td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Accu-jet pro</td>
			<td>Brand GmbH, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Beaker Glass 50 mL</td>
			<td>Schott AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Blunt cannula incl. Filter (5 &#181;m) 18G</td>
			<td>Becton Dickinson, USA</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Cell culture plate (12 well)</td>
			<td>Corning Inc., USA</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Colibri forceps</td>
			<td>Geuder AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Corneal scissors</td>
			<td>Geuder AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Eppendorf pipette</td>
			<td>Eppendorf AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Eye Bulb Holder</td>
			<td>L. Klein, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Eye scissors</td>
			<td>Geuder AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Folded Filter &#248; 185 mm</td>
			<td>Whatman, USA</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Hockey knife</td>
			<td>Geuder AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Laboratory Glass Bottle with cap 100 mL</td>
			<td>Schott AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Magnetic stir bar</td>
			<td>Carl Roth GmbH &#38; Co. KG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>MillexGV Filter (5 &#181;m)</td>
			<td>Merck Millopore Ltd., USA</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Needler holder</td>
			<td>Geuder AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Petri dishes</td>
			<td>VWR International, USA</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Pipette tips</td>
			<td>Sarstedt AG &#38; Co., Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Scalpel (single use), triangular blade</td>
			<td>Aesculap AG &#38; Co. KG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Serological pipette 10 mL</td>
			<td>Sarstedt AG &#38; Co., Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Serological pipette 5 mL</td>
			<td>Sarstedt AG &#38; Co., Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Sterile cups</td>
			<td>Greiner Bio-One, &#214;sterreich</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Sterile gloves</td>
			<td>Paul Hartmann AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Sterile surgical drape</td>
			<td>Paul Hartmann AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Stitch scissors</td>
			<td>Geuder AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Suture Ethilon 10-0 Polyamid 6</td>
			<td>Ethicon Inc., USA</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Syringe (5 mL)</td>
			<td>Becton Dickinson, USA</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>trephine &#248; 7.5 mm</td>
			<td>own production</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Tying forceps</td>
			<td>Geuder AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Weighing paper</td>
			<td>neoLab Migge GmbH, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Equipment &#38; Software</td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Binocular surgical microscope</td>
			<td>Carl Zeiss AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Camera mounted on microscope</td>
			<td>Olympus, Japan</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>CellSens Entry (software)</td>
			<td>Olympus, Japan</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Cold-light source</td>
			<td>Schott AG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Incubator</td>
			<td>Heraeus GmbH, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Inverted phase contrast microscope</td>
			<td>Olympus GmbH, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Magnetic stirrer with heating function</td>
			<td>IKA-Werke GmbH &#38; Co. KG, Germany</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>pH-meter pHenomenal</td>
			<td>VWR International, USA</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Photoshop CS2</td>
			<td>Adobe Systems, USA</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Precision scale</td>
			<td>Ohaus Europe GmbH, Switzerland</td>
			<td></td>
			<td></td>
		</tr>
	</tbody>
</table>

a porcine corneal endothelial organ culture model using split corneal buttons

Experimental research on corneal endothelial cells is associated with several difficulties. Human donor corneas are scarce and rarely available for experimental investigations as they are normally needed for transplantation. Endothelial cell cultures often do not translate well to in vivo situations. Due to the biostructural characteristics of non-human corneas, stromal swelling during cultivation induces substantial corneal endothelial cell loss, which makes it difficult to perform cultivation for an extended period of time. Deswelling agents such as dextran are used to counteract this response. However, they also cause significant endothelial cell loss. Therefore, an ex vivo organ culture model not requiring deswelling agents was established. Pig eyes from a local slaughterhouse were used to prepare split corneal buttons. After partial corneal trephination, the outer layers of the cornea (epithelium, bowman layer, parts of the stroma) were removed. This significantly reduces corneal endothelial cell loss induced by massive stromal swelling and Descemet&#39;s membrane folding throughout longer cultivation periods and improves general preservation of the endothelial cell layer. Subsequent complete corneal trephination was followed by the removal of the split corneal button from the remaining eye bulb and cultivation. Endothelial cell density was assessed at follow-up times of up to 15 days after preparation (i.e., days 1, 8, 15) using light microscopy. The preparation technique used allows a better preservation of the endothelial cell layer enabled by less stromal tissue swelling, which results in slow and linear decline rates in split corneal buttons comparable to human donor corneas. As this standardized organo-typically cultivated research model for the first time allows a stable cultivation for at least two weeks, it is a valuable alternative to human donor corneas for future investigations of various external factors with regards to their effects on the corneal endothelium.

The presented dissection technique implies partial removal of stromal tissue, resulting in a thinner cornea sample and thus less stromal swelling (Figure 1 and Figure 2). Less stromal swelling induces less shear and pinch forces that have a negative impact on the corneal endothelium, thus causing lower endothelial cell loss rates6. Split corneal buttons show a significantly better-preserved endothelial cel...

Watch this Scientific Journal Video about A Porcine Corneal Endothelial Organ Culture Model Using Split Corneal Buttons at JoVE.com

A Porcine Corneal Endothelial Organ Culture Model Using Split Corneal Buttons

Here, a step-by-step protocol for the preparation and cultivation of porcine split corneal buttons is presented. As this organo-typically cultivated organ culture model shows cell death rates within 15 days, comparable to human donor corneas, it represents the first model allowing long-term cultivation of non-human corneas without adding toxic dextran.

Experimental research on corneal endothelial cells is associated with several difficulties. Human donor corneas are scarce and rarely available for ...

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Research

JoVE Journal

Medicine

7.0K Views.  University Medical Center Hamburg-Eppendorf (UKE). Here, a step-by-step protocol for the preparation and cultivation of porcine split corneal buttons is presented. As this organo-typically cultivated organ culture model shows cell death rates within 15 days, comparable to human donor corneas, it represents the first model allowing long-term cultivation of non-human corneas without adding toxic dextran.

Video: A Porcine Corneal Endothelial Organ Culture Model Using Split Corneal Buttons

Corneal Confocal Microscopy: A Novel Non-invasive Technique to Quantify Small Fibre Pathology in Peripheral Neuropathies

The accurate quantification of peripheral neuropathy is important to define at risk patients, anticipate deterioration, and assess new therapies. Conventional methods assess neurological deficits and electrophysiology and quantitative sensory testing quantifies functional alterations to detect neuropathy. However, the earliest damage appears to be to the small fibres and yet these tests primarily assess large fibre dysfunction and have a limited ability to demonstrate regeneration and repair. The only techniques which allow a direct examination of unmyelinated nerve fibre damage and repair are sural nerve biopsy with electron microscopy and skin-punch biopsy. However, both are invasive procedures and require lengthy laboratory procedures and considerable expertise. Corneal Confocal microscopy is a non-invasive clinical technique which provides in-vivo imaging of corneal nerve fibres. We have demonstrated early nerve damage, which precedes loss of intraepidermal nerve fibres in skin biopsies together with stratification of neuropathic severity and repair following pancreas transplantation in diabetic patients. We have also demonstrated nerve damage in idiopathic small fibre neuropathy and Fabry's disease.

Corneal Confocal microscopy is a non-invasive clinical technique which may be used to quantify C fibre damage to diagnose and stratify patients with increasing neuropathic severity.

The accurate quantification of peripheral neuropathy is important to define at risk patients, anticipate deterioration, and assess new therapies. ...

Corneal Donor Tissue Preparation for Endothelial Keratoplasty

Over the past ten years, corneal transplantation surgical techniques have undergone revolutionary changes1,2. Since its inception, traditional full thickness corneal transplantation has been the treatment to restore sight in those limited by corneal disease. Some disadvantages to this approach include a high degree of post-operative astigmatism, lack of predictable refractive outcome, and disturbance to the ocular surface. The development of Descemet's stripping endothelial keratoplasty (DSEK), transplanting only the posterior corneal stroma, Descemet's membrane, and endothelium, has dramatically changed treatment of corneal endothelial disease. DSEK is performed through a smaller incision; this technique avoids 'open sky' surgery with its risk of hemorrhage or expulsion, decreases the incidence of postoperative wound dehiscence, reduces unpredictable refractive outcomes, and may decrease the rate of transplant rejection3-6.
Initially, cornea donor posterior lamellar dissection for DSEK was performed manually1 resulting in variable graft thickness and damage to the delicate corneal endothelial tissue during tissue processing. Automated lamellar dissection (Descemet's stripping automated endothelial keratoplasty, DSAEK) was developed to address these issues. Automated dissection utilizes the same technology as LASIK corneal flap creation with a mechanical microkeratome blade that helps to create uniform and thin tissue grafts for DSAEK surgery with minimal corneal endothelial cell loss in tissue processing.
Eye banks have been providing full thickness corneas for surgical transplantation for many years. In 2006, eye banks began to develop methodologies for supplying precut corneal tissue for endothelial keratoplasty. With the input of corneal surgeons, eye banks have developed thorough protocols to safely and effectively prepare posterior lamellar tissue for DSAEK surgery. This can be performed preoperatively at the eye bank. Research shows no significant difference in terms of the quality of the tissue7 or patient outcomes8,9 using eye bank precut tissue versus surgeon-prepared tissue for DSAEK surgery. For most corneal surgeons, the availability of precut DSAEK corneal tissue saves time and money10, and reduces the stress of performing the donor corneal dissection in the operating room. In part because of the ability of the eye banks to provide high quality posterior lamellar corneal in a timely manner, DSAEK has become the standard of care for surgical management of corneal endothelial disease.
The procedure that we are describing is the preparation of the posterior lamellar cornea at the eye bank for transplantation in DSAEK surgery (Figure 1).

Endothelial corneal transplantation is a surgical technique for treatment of posterior corneal diseases. Mechanical microkeratome dissection to prepare tissue results in thinner, more symmetric grafts with less endothelial cell loss and improved outcomes. Dissections can be performed at the eye bank prior to corneal transplantation surgery.

Over the past ten years, corneal transplantation surgical techniques have undergone revolutionary changes1,2. Since its inception, traditional full ...

An Alkali-burn Injury Model of Corneal Neovascularization in the Mouse

Under normal conditions, the cornea is avascular, and this transparency is essential for maintaining good visual acuity. Neovascularization (NV) of the cornea, which can be caused by trauma, keratoplasty or infectious disease, breaks down the so called &lsquo;angiogenic privilege' of the cornea and forms the basis of multiple visual pathologies that may even lead to blindness. Although there are several treatment options available, the fundamental medical need presented by corneal neovascular pathologies remains unmet. In order to develop safe, effective, and targeted therapies, a reliable model of corneal NV and pharmacological intervention is required. Here, we describe an alkali-burn injury corneal neovascularization model in the mouse. This protocol provides a method for the application of a controlled alkali-burn injury to the cornea, administration of a pharmacological compound of interest, and visualization of the result. This method could prove instrumental for studying the mechanisms and opportunities for intervention in corneal NV and other neovascular disorders.

Neovascularization (NV) of the cornea can complicate multiple visual pathologies. Utilizing a controlled, alkali-burn injury model, a quantifiable level of corneal NV can be produced for mechanistic study of corneal NV and evaluation of potential therapies for neovascular disorders.

Under normal conditions, the cornea is avascular, and this transparency is essential for maintaining good visual acuity. Neovascularization (NV) of the ...

Murine Corneal Transplantation: A Model to Study the Most Common Form of Solid Organ Transplantation

Corneal transplantation is the most common form of organ transplantation in the United States with between 45,000 and 55,000 procedures performed each year. While several animal models exist for this procedure and mice are the species that is most commonly used. The reasons for using mice are the relative cost of using this species, the existence of many genetically defined strains that allow for the study of immune responses, and the existence of an extensive array of reagents that can be used to further define responses in this species. This model has been used to define factors in the cornea that are responsible for the relative immune privilege status of this tissue that enables corneal allografts to survive acute rejection in the absence of immunosuppressive therapy. It has also been used to define those factors that are most important in rejection of such allografts. Consequently, much of what we know concerning mechanisms of both corneal allograft acceptance and rejection are due to studies using a murine model of corneal transplantation. In addition to describing a model for acute corneal allograft rejection, we also present for the first time a model of late-term corneal allograft rejection.

Mice have been used as a model for studying many forms of transplantation, including corneal transplantation. We describe in this report a murine model for both acute and late-term corneal transplantation.

Corneal transplantation is the most common form of organ transplantation in the United States with between 45,000 and 55,000 procedures performed each ...

Corneal Donor Tissue Preparation for Descemet's Membrane Endothelial Keratoplasty

Descemet&#8217;s Membrane Endothelial Keratoplasty (DMEK) is a form of corneal transplantation in which only a single cell layer, the corneal endothelium, along with its basement membrane (Descemet&#39;s membrane) is introduced onto the recipient&#39;s posterior stroma3. Unlike Descemet&#8217;s Stripping Automated Endothelial Keratoplasty (DSAEK), where additional donor stroma is introduced, no unnatural stroma-to-stroma interface is created. As a result, the natural anatomy of the cornea is preserved as much as possible allowing for improved recovery time and visual acuity4. Endothelial Keratoplasty (EK) is the procedure of choice for treatment of endothelial dysfunction. The advantages of EK include rapid recovery of vision, preservation of ocular integrity and minimal refractive change due to use of a small, peripheral incision1. DSAEK utilizes donor tissue prepared with partial thickness stroma and endothelium. The rapid success and utilization of this procedure can be attributed to availability of eye-bank prepared precut tissue. The benefits of eye-bank preparation of donor tissue include elimination of need for specialized equipment in the operating room and availability of back up donor tissue in case of tissue perforation during preparation. In addition, high volume preparation of donor tissue by eye-bank technicians may provide improved quality of donor tissue. DSAEK may have limited best corrected visual acuity due to creation of a stromal interface between the donor and recipient cornea. Elimination of this interface with transplantation of only donor Descemet&#39;s membrane and endothelium in DMEK may improve visual outcomes and reduce complications after EK5. Similar to DSAEK, long term success and acceptance of DMEK is dependent on ease of availability of precut, eye-bank prepared donor tissue. Here we present a stepwise approach to donor tissue preparation which may reduce some barriers eye-banks face in providing DMEK grafts.

Endothelial keratoplasty is a surgical technique continuously evolving as advancements result in transplantation of thinner grafts with each succession1. Here we present a technique for controlled manual tissue dissection to allow safe and repeatable separation of endothelium and Descemet&#39;s membranes from donor corneoscleral buttons for transplantation2.

Descemet&#8217;s Membrane Endothelial Keratoplasty (DMEK) is a form of corneal transplantation in which only a single cell layer, the corneal endothelium, ...

Technique of Porcine Liver Procurement and Orthotopic Transplantation using an Active Porto-Caval Shunt

The success of liver transplantation has resulted in a dramatic organ shortage. Each year, a considerable number of patients on the liver transplantation waiting list die without receiving an organ transplant or are delisted due to disease progression. Even after a successful transplantation, rejection and side effects of immunosuppression remain major concerns for graft survival and patient morbidity. 
Experimental animal research has been essential to the success of liver transplantation and still plays a pivotal role in the development of clinical transplantation practice. In particular, the porcine orthotopic liver transplantation model (OLTx) is optimal for clinically oriented research for its close resemblance to human size, anatomy, and physiology. 
Decompression of intestinal congestion during the anhepatic phase of porcine OLTx is important to guarantee reliable animal survival. The use of an active porto-caval-jugular shunt achieves excellent intestinal decompression. The system can be used for short-term as well as long-term survival experiments. The following protocol contains all technical information for a stable and reproducible liver transplantation model in pigs including post-operative animal care.

Experimental animal research plays a pivotal role in the development of clinical transplantation practice. The porcine orthotopic liver transplantation model (OLTx) closely resembles human conditions and is frequently used in clinically oriented research. The following protocol contains all information for a reliable porcine OLTx model using an active porto-caval-jugular shunt.

The success of liver transplantation has resulted in a dramatic organ shortage. Each year, a considerable number of patients on the liver transplantation ...

Heterotopic Renal Autotransplantation in a Porcine Model: A Step-by-Step Protocol

Kidney transplantation is the treatment of choice for patients suffering from end-stage renal disease. It offers better life expectancy and higher quality of life when compared to dialysis. Although the last few decades have seen major improvements in patient outcomes following kidney transplantation, the increasing shortage of available organs represents a severe problem worldwide. To expand the donor pool, marginal kidney grafts recovered from extended criteria donors (ECD) or donated after circulatory death (DCD) are now accepted for transplantation. To further improve the postoperative outcome of these marginal grafts, research must focus on new therapeutic approaches such as alternative preservation techniques, immunomodulation, gene transfer, and stem cell administration.
Experimental studies in animal models are the final step before newly developed techniques can be translated into clinical practice. Porcine kidney transplantation is an excellent model of human transplantation and allows investigation of novel approaches. The major advantage of the porcine model is its anatomical and physiological similarity to the human body, which facilitates the rapid translation of new findings to clinical trials. This article offers a surgical step-by-step protocol for an autotransplantation model and highlights key factors to ensure experimental success. Adequate pre- and postoperative housing, attentive anesthesia, and consistent surgical techniques result in favorable postoperative outcomes. Resection of the contralateral native kidney provides the opportunity to assess post-transplant graft function. The placement of venous and urinary catheters and the use of metabolic cages allow further detailed evaluation. For long-term follow-up studies and investigation of alternative graft preservation techniques, autotransplantation models are superior to allotransplantation models, as they avoid the confounding bias posed by rejection and immunosuppressive medication.

Porcine models of organ transplantation provide an important platform to study mechanisms of organ preservation. This article describes a heterotopic porcine renal autotransplantation model, which allows investigating new approaches to improve the outcome of transplantation using marginal kidney grafts.

Kidney transplantation is the treatment of choice for patients suffering from end-stage renal disease. It offers better life expectancy and higher quality ...

Corneal Epithelial Abrasion with Ocular Burr As a Model for Cornea Wound Healing

The murine cornea provides an excellent model to study wound healing. The cornea is the outermost layer of the eye, and thus is the first defense to injury. In fact, the most common type of eye injury found in clinic is a corneal abrasion. Here, we utilize an ocular burr to induce an abrasion resulting in removal of the corneal epithelium in vivo on anesthetized mice. This method allows for targeted and reproducible epithelial disruption, leaving other areas intact. In addition, we describe the visualization of the abraded epithelium with fluorescein staining and provide concrete advice on how to visualize the abraded cornea. Then, we follow the timeline of wound healing 0, 18, and 72 h after abrasion, until the wound is re-epithelialized. The epithelial abrasion model of corneal injury is ideal for studies on epithelial cell proliferation, migration and re-epithelialization of the corneal layers. However, this method is not optimal to study stromal activation during wound healing, because the ocular burr does not penetrate to the stromal cell layers. This method is also suitable for clinical applications, for example, pre-clinical test of drug effectiveness.

This protocol describes a method to inflict an abrasion to the ocular surface of the mouse, and to follow the wound healing process thereafter. The protocol takes advantage of an ocular burr to partially remove the surface epithelium of the eye in anaesthetized mice.

The murine cornea provides an excellent model to study wound healing. The cornea is the outermost layer of the eye, and thus is the first defense to ...

Ex Vivo Corneal Organ Culture Model for Wound Healing Studies

The cornea has been used extensively as a model system to study wound healing. The ability to generate and utilize primary mammalian cells in two dimensional (2D) and three dimensional (3D) culture has generated a wealth of information not only about corneal biology but also about wound healing, myofibroblast biology, and scarring in general. The goal of the protocol is an assay system for quantifying myofibroblast development, which characterizes scarring. We demonstrate a corneal organ culture ex vivo model using pig eyes. In this anterior keratectomy wound, corneas still in the globe are wounded with a circular blade called a trephine. A plug of approximately 1/3 of the anterior cornea is removed including the epithelium, the basement membrane, and the anterior part of the stroma. After wounding, corneas are cut from the globe, mounted on a collagen/agar base, and cultured for two weeks in supplemented-serum free medium with stabilized vitamin C to augment cell proliferation and extracellular matrix secretion by resident fibroblasts. Activation of myofibroblasts in the anterior stroma is evident in the healed cornea. This model can be used to assay wound closure, the development of myofibroblasts and fibrotic markers, and for toxicology studies. In addition, the effects of small molecule inhibitors as well as lipid-mediated siRNA transfection for gene knockdown can be tested in this system.

A protocol for an ex vivo corneal organ culture model useful for wound healing studies is described. This model system can be used to assess the effects of agents to promote regenerative healing or drug toxicity in an organized 3D multicellular environment.

The cornea has been used extensively as a model system to study wound healing. The ability to generate and utilize primary mammalian cells in two ...

Development of a Noninvasive, Laser-Assisted Experimental Model of Corneal Endothelial Cell Loss

Nd:YAG lasers have been used to perform noninvasive intraocular surgery, such as capsulotomy for several decades now. The incisive effect relies on the optical breakdown at the laser focus. Acoustic shock waves and cavitation bubbles are generated, causing tissue rupture. Bubble sizes and pressure amplitudes vary with pulse energy and position of the focal point. In this study, enucleated porcine eyes were positioned in front of a commercially available Nd:YAG laser. Variable pulse energies as well as different positions of the focal spots posterior to the cornea were tested. Resulting lesions were evaluated by two-photon microscopy and histology to determine the best parameters for an exclusive detachment of corneal endothelial cells (CEC) with minimum collateral damage. The advantages of this method are the precise ablation of CEC, reduced collateral damage, and above all, the non-contact treatment.

Here, we present a protocol to detach corneal endothelial cells (CEC) from Descemet&#8217;s membrane (DM) using a neodymium:YAG (Nd:YAG) laser as an ex vivo disease model for bullous keratopathy (BK).

Nd:YAG lasers have been used to perform noninvasive intraocular surgery, such as capsulotomy for several decades now. The incisive effect relies on the ...