Image-Guided Optical Coherence Tomography to Assess Structural Changes in Rodent Retinas

Summary

The protocol presented here details the procedures of data collection and data analysis for image-guided optical coherence tomography (OCT) and demonstrates its application in multiple rodent models of ocular diseases.

Abstract

Ocular diseases, such as age-related macular degeneration, glaucoma, retinitis pigmentosa, and uveitis, are always accompanied by retinal structural changes. These diseases affecting the fundus always exhibit typical abnormalities in certain cell types in the retina, including photoreceptor cells, retinal ganglion cells, cells in the retinal blood vessels, and cells in the choroidal vascular cells. Noninvasive, highly efficient, and adaptable imaging techniques are required for both clinical practice and basic research. Image-guided optical coherence tomography (OCT) satisfies these requirements because it combines fundus photography and high-resolution OCT, providing an accurate diagnosis of tiny lesions as well as important changes in the retinal architecture. This study details the procedures of data collection and data analysis for image-guided OCT and demonstrates its application in rodent models of choroidal neovascularization (CNV), optic nerve crush (ONC), light-induced retinal degeneration, and experimental autoimmune uveitis (EAU). This technique helps researchers in the eye field to identify rodent retinal structural changes conveniently, reliably, and tractably.

Introduction

Ocular diseases affecting the fundus always exhibit typical abnormalities in certain cell types in the retina, such as photoreceptor cells, retinal ganglion cells, cells in the retinal blood vessels, and cells in the choroidal blood vessels, which may subsequently influence the visual acuity of patients¹. To avoid irreversible visual impairment, timely diagnoses and appropriate treatments are required¹. Optical coherence tomography (OCT) has been widely used in the clinic to evaluate a range of ocular diseases, including age-related macular degeneration, retinitis pigmentosa, glaucoma, uveitis, and retinal detachment, among others^2,3,4. This kind of noninvasive, highly efficient, and adaptable imaging technique is also needed for the timely evaluation of the disease conditions in experimental animals^5,6,7,8,9,10.

Image-guided optical coherence tomography (OCT) uses interferometry to produce cross-sectional images of animal retinas at 1.8 µm longitudinal resolution and 2 µm axial resolution. It has at least three advantages in the investigation of retinal architectural changes^{2,3,4,5,6,7,8,9,10}. First, it is a noninvasive technique that allows researchers to dynamically follow the location of interest in the same animal retina^5,6,7,8,9,10. Second, this trait substantially reduces the sample size for every experiment³. Meanwhile, it saves considerable time and effort in research projects^{2,3,4,5,6,7,8,9,10}. Third, image-guided OCT acquires colorful fundus images while capturing OCT images, thus providing accurate and reliable results for users.

This manuscript describes the procedures of image collection and data analysis for image-guided OCT and elaborates on its application in mouse and rat models of choroidal neovascularization (CNV)^11,12, optic nerve crush (ONC)^13,14,15,16, light-induced retinal degeneration^{17,18,19,20,21}, and experimental autoimmune uveitis (EAU)^22,23. With this versatile technique, researchers can capture high-resolution OCT images as well as fundus images conveniently and efficiently.

Protocol

All the animal procedures conformed to the Association for Research on Vision and Ophthalmology's statement on the Use of Animals in Ophthalmic and Vision Research and were approved by the Institutional Animal Care and Use Committee of Wenzhou Medical University (WMU). The rats and mice were given free access to water and food with an environmental light intensity of 18 lux on a 12 h dark/light cycle.

1. Preparation of the ocular animal models

1. Mouse laser-induced choroidal neovascularization (CNV) model^11,12
   1. Anesthetize 4-week-old female mice (C57BL/6J background) with ketamine and xylazine, and dilate the pupils with tropicamide phenylephrine eye drops following step 3.2. Consider the mouse properly anesthetized when no movement is detected after pinching the toe.
   2. Engage the light-source box, the software, and the laser box (wavelength: 532 nm), with the output energy adjusted to 100 mW and the duration to 100 ms.
   3. Place the mouse on the experimental platform and adjust the position of the mouse and the platform until the view of the mouse fundus is clear.
   4. Press the Laser ON button on the screen of the laser box and adjust the focus of the red laser reference spot. Move the laser reference spot and adjust it to one to two papillary diameters away from the optic disc. Operate the foot pedal to cause laser damage.
   5. Conduct an immediate check to determine whether a vaporizing bubble occurred immediately after the hit, which is a sign of successful laser damage. Generate three to five laser spots for each eye.
2. Mouse optic nerve crush (ONC) model^13,14,15,16
   1. Anesthetize female mice (C57BL/6J background) at postnatal day (P) 21 to P35 following step 3.2. Consider the mouse properly anesthetized when no movement is detected after pinching the toe.
   2. Place the mouse under a surgical microscope, and incise the conjunctiva of one eye using spring scissors, ensuring the size of the conjunctiva incision is approximately 1 mm.
   3. Expose the intraorbital optic nerve, and crush with fine forceps for 5 s at 0.5 mm away from the optic disc. While doing this, gently deflect the orbital muscles and the other tissues, and place them aside. Avoid damage to any blood vessels in the surgical eye.
      NOTE: Be careful, as the eyeball will swing when touching or plucking the white bunchy optic nerve.
   4. Apply ophthalmic ointment postoperatively to avoid corneal dryness.
3. Mouse light-induced retinal degeneration (LIRD) model^{17,18,19,20,21}
   1. Preparations before the experiment: Enclose the mouse cages (30 cm x 18 cm x 13 cm) with aluminum foil and an iron mesh cover. Place each cage in a paper box (52 cm x 35 cm x 30 cm) with a white light on the top.
   2. Dark-adapt 6-week-old male mice (BALB/c) overnight in the dark room, and then dilate the eyes using tropicamide phenylephrine eye drops in each eye. Fully dilate the pupil until 3/4 of the cornea area is not covered by the iris; this often takes no more than 3 min.
   3. Illuminate the mice with 10,000 lux white light for 2 h. Keep the mice in the dark overnight postoperatively, and then return to normal dark-light environments. To ensure an effective light stimulus, keep one mouse in the cage at all times.
4. Rat experimental autoimmune uveitis (EAU) model
   1. Preparations before the experiment: Emulsify 2.5 mg of hIRBP161-180 in complete Freund's adjuvant (1:1 weight/volume) with 2.5 mg/mL Mycobacterium tuberculosis H37Ra^22,23.
   2. Inject 100 µL of emulsion subcutaneously into the left footpad of each Lewis male rat (about 180 g).

2. OCT module setup

1. Connect the optical fiber and the OCT control cable between the OCT scan head and the OCT engine (Figure 1A). Align the notch on the fiber with a slot on the connector, and gently insert the tip until it is seated (Figure 1B).
   NOTE: Before connecting the control cable, turn the power switch of the OCT engine OFF. The optical fiber is very fragile, so avoid both ends of the fiber tip (Figure 1C). Assembling and disassembling the OCT scan head and the fiber/cable should be avoided if this module is under frequent use.
2. Thread the mouse or rat OCT objective lens to the front of the machine body (Figure 1A). Place the OCT scan head onto the OCT lens, with the M-R focus indicator facing away from the machine body (Figure 1A).
3. Secure the OCT scan head with two thumbscrews: one on the lens and one on the camera body. Fix the scan head tightly.
4. Turn on the main power switch, followed by the camera light, and then the OCT software.
   ​NOTE: The camera needs some time to boot up for the computer to find it.

3. Animal preparation for OCT experiments

1. At 10 min before the OCT experiments, instill tropicamide phenylephrine eye drops in the animal's eyes, and wipe away excess eye drops using a clean towel.
2. At 5 min before the experiment, inject 200 µL of the anesthetic solution into the mouse, and inject 2.0 mL into the rat intraperitoneally. Consider the mouse/rat properly anesthetized when no movement is detected after pinching the toe.
   NOTE: The anesthetic solutions were composed of ketamine (12 mg/mL) and xylazine (1 mg/mL for the mouse and 2 mg/mL for the rat) in saline; typically, 10 µL of anesthetic solution per 1 g of animal body mass is applied. The solutions were stored at 4 °C for a maximum of 2 weeks.
3. Once anesthesia is administered, lubricate the cornea with gel ointment to avoid ocular surface dryness.

4. Image-guided OCT Imaging

NOTE: The software interface was divided into three parts: brightfield image, OCT control tabs, and OCT display (Figure 2).

1. When looking at the brightfield image, type the annotation of the animal information if needed.
2. Toggle the Beam Position Controls ON or OFF using the check box to capture a brightfield image with or without the line overlay on the image.
3. To place the scanning beam more precisely, use the Position Nudge arrows for fine control to direct it up, down, left, or right. Choose the thickness values and color, and choose an angle for the beam targeting the location of interest (e.g., thick, black, and 0). Drag the gain value to 14 db.
4. Go to the OCT control tabs. From the menu, select File/File_Settings, and then create a path to where the OCT and fundus images will be saved.
5. Specify the scan type, size, and animal (rat or mouse); choose Eye, left or right, and Imaging Retina.
   NOTE: OCT can capture line, circle, and 3D volume scan types at full, half, quarter, and eighth sizes.
6. Set the image controls. Adjust the values: 60 for the contrast, 100 for the gamma , and 0 for the brightness.
7. Place the mouse on the experimental platform and adjust the position of the mouse and platform until the view of the mouse fundus is clear. Finely adjust the position to localize the optic disc in the center.
8. Adjust the reference arm to 850 for mice and 830 for rats at the beginning, and then finely adjust the position by clicking the <-1 or +1> buttons. Adjust the OCT image horizontally, and then move the OCT image to the top 1/3 of the full view.
9. Move the polarization slider to adjust the brightness of the signal through the retina, if needed.
10. After observing a clear and stable OCT image as well as the fundus image, set the number of frames (usually 20, 50, 80, or 100), and then press Average.
    NOTE: It takes several seconds to capture the OCT images. A larger number of frames means the image capture takes longer to finish but produces a higher-quality captured image.
11. Press Save to save the OCT and fundus images, and then click Restart to capture another sample.
    ​NOTE: The animals were allowed to recover on a 37 °C heating plate before awakening. The animals were not left unattended until they had regained sufficient consciousness to maintain sternal recumbency. The animals that had undergone treatment were not returned to the raising system of other animals until fully recovered.

5. Thickness measurement and quantitative analysis

NOTE: This OCT has built-in analysis software. OCT images can be segmented and analyzed using this software (Figure 3).

1. Open the analysis software and open an OCT image that needs to be analyzed.
2. Choose the number of layers, and then press Get Initial Layers (Figure 3A). The software will draw the layers automatically.
3. Click the Pencil icon, and then move the dots on the target layer to finely adjust the layer (Figure 3A, B). Modify all the layers carefully one by one.
   NOTE: Adding more layers is doable. Click on the Plus icon, draw several dots over the OCT image, and then press the Tick icon. A new layer will be created.
4. Once fine adjustments of the layers are completed, export the detailed values (CSV format) and different image types of the segmented OCT (Figure 3A).
   NOTE: It is possible to export different image types, including layers, thickness, thickness map, layers without OCT, and screen grabs. The value in the middle that overlaps with the optic nerve of every image needs to be abandoned and set as zero since there is no retinal layer there.

Results

Image-guided OCT can be used to monitor the development of the laser spot in laser-induced choroidal neovascularization (CNV) in mice. As shown in Figure 1, the newborn blood vessels passed through Bruch's membrane as well as the retinal pigment epithelium (RPE) layer and formed a fibrotic scar after laser injury^11,12. This lesion spot could be captured under either full-size scanning (Figure 4A) or ...

Discussion

This protocol provides instructions for the image collection and thickness measurement of image-guided OCT. By demonstrating the four most popular rodent models of ocular diseases, the researchers found that image-guided OCT provided excellent performance in examining drastic retinal structural alterations. In fact, with high-resolution images, tiny lesions can be found easily in OCT images as well. With the aid of image-guided OCT, a group in the laboratory also found abnormal hyperreflectivity spots within the OPL in a...

Materials

Name	Company	Catalog Number	Comments
BALB/c mouse	Beijing Vital River Laboratory Animal Technology Co., Ltd		Animal model preparations
C57BL/6JNifdc mouse	Beijing Vital River Laboratory Animal Technology Co., Ltd		Animal model preparations
Carbomer Eye Gel	Fabrik GmbH Subsidiary of Bausch & Lomb		Moisten the cornea
Complete Freund’s adjuvant	Sigma	F5881	EAU experiment
Experimental platform	Phoenix Technology Group		Animal model preparations
hIRBP161-180	Shanghai Sangon Biological Engineering Technology & Services Co., Ltd.		EAU experiment
Ketamine	Ceva Sante Animale		General anesthesia
Laser box	Haag-Streit Group	Merilas 532α	Animal model preparations
Lewis rat	Beijing Vital River Laboratory Animal Technology Co., Ltd		Animal model preparations
Mycobacterium Tuberculosis H37RA	Sigma	344289	EAU experiment
Phoneix Micron IV with image-guided OCT and image-guided laser	Phoenix Technology Group		Animal model preparations
Tissue forceps	Suzhou Mingren Medical Instrument Co., Ltd	MR-F101A-5	Animal model preparations
Tropicamide Phenylephrine Eye Drops	SANTEN OY, Japan		Eye dilatation
Vannas scissors	Suzhou Mingren Medical Instrument Co., Ltd	MR-S121A	Animal model preparations
Xylazine	Ceva Sante Animale		General anesthesia