Implantation and Recording of Wireless Electroretinogram and Visual Evoked Potential in Conscious Rats

Jason Charng; Zheng He; Bang Bui; Algis Vingrys; Magnus Ivarsson; Rebecca Fish; Rachel Gurrell; Christine Nguyen

doi:10.3791/54160

JoVE Journal > Behavior

Sciences du comportement

Implantation and Recording of Wireless Electroretinogram and Visual Evoked Potential in Conscious Rats

Published: June 29, 2016

doi:

10.3791/54160

Jason Charng¹, Zheng He¹, Bang Bui¹, Algis Vingrys¹, Magnus Ivarsson¹, Rebecca Fish², Rachel Gurrell², Christine Nguyen¹

¹Department of Optometry and Vision Sciences,University of Melbourne, ²Pfizer Neusentis

Summary

We show surgical implantation and Recording procedures to measure visual electrophysiological signals from the eye (electroretinogram) and brain (visual evoked potential) in conscious rats, which is more analogous to the human condition where recordings are conducted without anesthesia confounds.

Abstract

The full-field electroretinogram (ERG) and visual evoked potential (VEP) are useful tools to assess retinal and visual pathway integrity in both laboratory and clinical settings. Currently, preclinical ERG and VEP measurements are performed with anesthesia to ensure stable electrode placements. However, the very presence of anesthesia has been shown to contaminate normal physiological responses. To overcome these anesthesia confounds, we develop a novel platform to assay ERG and VEP in conscious rats. Electrodes are surgically implanted sub-conjunctivally on the eye to assay the ERG and epidurally over the visual cortex to measure the VEP. A range of amplitude and sensitivity/timing parameters are assayed for both the ERG and VEP at increasing luminous energies. The ERG and VEP signals are shown to be stable and repeatable for at least 4 weeks post surgical implantation. This ability to record ERG and VEP signals without anesthesia confounds in the preclinical setting should provide superior translation to clinical data.

Introduction

The ERG and VEP are minimally invasive in vivo tools to assess the integrity of retinal and visual pathways respectively in both the laboratory and clinic. The full-field ERG yields a characteristic waveform which can be broken down into different components, with each element representing different cell classes of the retinal pathway^1,2. The classic full-field ERG waveform consists of an initial negative slope (a-wave), which has been shown to represent photoreceptor activity post light exposure^2-4. The a-wave is followed by a substantial positive waveform (b-wave) which reflects electrical activity of middle retina, predominantly the ON-bipolar cells^5-7. Furthermore, one can vary luminous energy and inter-stimulus-interval to isolate cone from rod responses⁸.

The flash VEP represents electrical potentials of the visual cortex and brain stem in response to retinal light stimulation^9,10. This waveform can be broken down into early and late components, with the early component reflecting activity of neurons of the retino-geniculo-striate pathway^11-13 and the late component representing cortical processing performed in various V1 laminae in rats^11,13. Therefore simultaneous measurement of the ERG and VEP returns comprehensive assessment of the structures involved in the visual pathway.

Currently, in order to record electrophysiology in animals, anesthesia is employed to enable stable placement of electrodes. There have been attempts to measure ERG and VEP in conscious rats^14-16 but these studies employed a wired setup, which can be cumbersome and may lead to animal stress by restricting animal movement and natural behavior¹⁷. With recent advances in wireless technology including improved miniaturization and battery life, it is now possible to implement a telemetry approach for ERG and VEP recording, decreasing the stress associated with wired recordings and improving long term viability. Fully internalized stable implantations of telemetry probes have proven to be successful for chronic monitoring of temperature, blood pressure¹⁸, activity¹⁹ as well as electroencephalography²⁰. Such advances in technology will also assist with repeatability and stability of conscious recordings, increasing the platform's utility for chronic studies.

Protocol

Ethics statement: Animal experiments were conducted in accordance with the Australian Code for the Care and Use of Animals for Scientific Purposes (2013). Animal ethics approval was obtained from the Animal Ethics Committee, University of Melbourne. The materials herein are for laboratory experiments only, and not intended for medical or veterinary use.

1. Preparing Electrodes

Note: A three channel transmitter is used for surgical implantation which enables 2 ERG and 1 VEP recording to be conducted simultaneously. The three active and three inactive electrodes need to be pre-fashioned into a ring shape before implantation in order to attach to the eye. For identification purposes, the manufacturer has enclosed active electrodes in half white, half colored plastic sheaths while inactive electrodes are covered in full colored sheaths. The ground electrode (clear plastic sheath) is left unaltered. For all active and inactive electrodes conduct steps 1.1, 1.2, 1.3 and 1.7.

Untwist the double stranded stainless steel electrode with two fine tipped pliers.
Trim one of the stainless steel strands (approximately 1 cm from the tip), leaving a single longer straight strand remaining to shape the ring electrode.
Fold the single stainless steel strand back onto itself and twist, forming a smooth ring at the tip of the electrode.
For the ERG active electrodes fashion this loop ~ 0.2 – 0.5 mm in diameter by twisting the base of the loop (for the purpose described here, shape two active electrodes in this way to record ERG from both eyes), and for the ERG inactive and VEP electrodes make the loop diameter ~ 0.8 mm diameter (in this example, do this for one active VEP electrode and all three inactive electrodes).
Hook the circular VEP active electrode around a stainless steel screw (diameter 0.7 mm, length 3 mm) so the electrode rests against the screw head.
Hook the 3 inactive electrodes (2 ERG, 1 VEP) around a second stainless steel screw (diameter 0.7 mm, length 3 mm).
Pull the plastic sleeve forward over the sharp ends of the two stainless steel strand to reduce irritation.
Sterilize the telemetry transmitters by soaking in 2% glutaraldehyde for more than 10 hr at approximately 25 °C. Then rinse the transmitter with sterile saline 3 times.

2. Transmitter Implantation

Animal Preparation
1. Disinfect the surgical area prior to experimentation by cleaning with 70% ethanol. Autoclave all surgical equipment before use and maintain equipment in chlorhexidine when not in use during surgery. Cover the animal with a surgical drape during surgery to maintain a sterile environment. Ensure all experimenters wear surgical masks, sterile gloves and gowns.
2. Induce anesthesia with 1.5 – 2% isoflurane, at a flow rate of 3 L/min and maintained at 1.5 – 2 % at 2 L/min throughout the surgery. Confirm sufficient depth of anesthesia by absence of a pedal reflex upon pinching the muscle between the toes.
3. Shave a 40 mm x 30 mm area over the abdomen from above the groin to the sternum.
4. Shave a 30 mm x 20 mm area over the forehead, posterior to the eyes and anterior to the ears.
5. Disinfect the two shaved areas. For the forehead area disinfect with 10% povidone-iodine three times (avoid the use of alcohol-based antiseptics for area near the eye, being consistent with the Standard of Practice set out by the Association of Surgical Technologists). Over the abdomen disinfect with 10% povidone iodine and 70% ethanol.
6. Apply 1 drop of proxymetacaine to the cornea for additional topical anesthesia.
7. Apply 1 drop of carboxymethylcellulose sodium to the cornea to prevent drying of the eyes.
Surgical implantation
1. Make a 10 mm incision on the head along the vertical midline between the ears with a surgical scalpel.
2. Make a 5 mm incision on the abdomen through the skin layer along the midline below the sternum.
3. Tunnel a 5 mm diameter cannula subcutaneously from the abdomen incision to the head incision.
4. Feed the electrode wires (3 active and 3 inactive) of the transmitter through the cannula from the abdomen to the head.
5. Leave the reference electrode with the transmitter base and cover the electrode tip with aseptic gauze.
6. Cover the electrode tips (3 active and 3 inactive) with aseptic gauze.
7. Secure the rat's head to a stereotaxic platform.
8. Extend the forehead incision to 30mm in length with surgical scissors.
9. Expose surgical area by retracting loose skin with 2 sutures (3 – 0) at ~ 3 and 9 o'clock.
10. Scrape off the periosteum overlying the skull using sterilized gauze to expose bregma, lambda and midline sutures.
11. Drill two holes through the skull at the VEP active (7 mm ventral to bregma 3 mm lateral to midline) and inactive (5 mm rostral to bregma on the midline) stereotaxic co-ordinates.
12. Attach VEP active and inactive electrodes with pre-attached stainless steel screws (diameter 0.7 mm, length 3 mm) to the skull with a small screw-driver to ~ 1 mm in depth into the premade holes. This anchors the screw to the bone without damaging the underlying cortical tissue.
13. To implant the ERG active electrodes use an 8 – 0 suture to temporarily retract the upper eyelid.
14. Insert a 16 to 21 G cannula subcutaneously from behind the eye through to the superior conjunctival fornix.
15. Remove the guiding needle.
16. Feed the active electrode through the shortened plastic catheter from the forehead towards the eye. Then remove the plastic catheter.
17. Use a temporary suture (8 – 0), which is threaded through the electrode loop, to prevent the electrode from retracting back into the tunnel.
18. Make a 0.5 mm incision on the superior conjunctiva at 12 o'clock, 1 mm behind limbus. Use blunt dissection to expose the underlying sclera.
19. Implant an 8 – 0 or 9 – 0 suture immediately behind the limbus at half scleral thickness.
20. Remove temporary suture from ERG active electrode.
21. Anchor the ERG active electrode to the half scleral thickness suture by tying 3 consecutive knots ensuring the tip of the electrode is situated close to the limbus.
22. Close the conjunctival flap using 1 to 2 interrupted sutures (8 – 0 to 9 – 0). Ensure that the conjunctiva completely covers the ERG electrode to improve comfort.
23. Remove the eyelid retracting suture.
24. Repeat the procedure for the contralateral eye.
25. Apply cyanoacrylate gel over the skull to secure all stainless screws and electrode wires. Ensure the ERG active electrodes are not pulled too tight before securing to enable eye movements.
26. Close the head wound using a non-absorbable 3 – 0 suture.
27. Rotate rodent to expose abdominal area. Lengthen the abdominal dermal incision to 40 mm along the linea alba with surgical scissors.
28. Make a 35 mm incision through the inner muscle wall to expose the inner abdominal cavity.
29. Using two sutures (3 – 0) attach the transmitter body to the animal's right hand side inner abdominal wall. Avoid contacting the liver.
30. Loop the ground electrode and secure in this shape with a suture (3 – 0). Place it free-floating in the abdominal cavity.
31. Close the peritoneum using a continuous suture (3 – 0).
32. Close the skin incision using interrupted sutures (3 – 0).
Post-operative care
1. Monitor the animal until it has regained sufficient consciousness to maintain sternal recumbency. House the animal singly following the surgery.
2. Administer carprofen subcutaneously for analgesia (5 mg/kg) once a day for 4 days.
3. Add prophylactic oral antibiotics (Enrofloxin, 5 mg/kg) to the drinking water for 7 days post-surgery.
4. Apply an anti-inflammatory ointment to skin incision sites to reduce irritation for the first 7 days post-surgery.

3. Conduct ERG and VEP Recordings in Conscious Rats

Dark adapt animal for 12 hr prior to ERG and VEP recordings
Conduct all experimental manipulations under dim red illumination (17.4 cd.m^-2, λ_max = 600 nm)
Apply topical anesthesia (0.5% proxymetacaine) and dilating (0.5% tropicamide) drops to the cornea.
Guide the conscious rodent into a custom made, clear restrainer.
Note: The length of this plastic tube can be adjusted to accommodate different sized rats with the overall diameter fixed at 60 mm. The front end of the device is tapered to minimize head movement and contains perforations to enable normal breathing. This tapered front allows alignment and stabilization of the rat's head and eyes to the opening of the Ganzfeld sphere. Note that the rodent has been acclimatized to the restrainer (3 to 5 occasions) prior to surgery.
Place the rodent in front of the Ganzfeld bowl with the eyes aligned with the opening of the bowl.
Turn on indwelling transmitter by passing a magnet within ~ 5 cm of the transmitter. Verify that the transmitter is on by checking the LED status light on the receiver base.
Collect signals over a range of luminous energies (i.e., -5.6 to 1.52 log cd.s.m^-2) as described previously²¹. Briefly, average more signals at the dimmer light levels (~ 80 repeats) and less at the brighter luminous energies (~ 1 repeat). Gradually lengthen the interstimulus interval from 1 to 180 seconds from dimmest to the brightest light level.
To isolate the ERG rod and cone responses utilize a twin-flash paradigm⁸. For example, initiate two flashes at 1.52 log cd.s.m^-2 with a 500 msec inter-stimulus interval in-between.
To record VEP signals, average 20 repeats at the brighter luminous energies (i.e., 1.52 log cd.s.m^-2, 5 sec inter-stimulus interval).
To evaluate implant stability, which is assessed by signal variability over time, conduct ERG and VEP recordings 7, 10, 14, 21 and 28 days post-surgery.
Following experimental period, euthanize rats via intracardial injection of pentobarbiturate (1.5 ml/kg) after ketamine:xylazine anesthesia (12:1 mg/kg).

Representative Results

The photoreceptor response is analyzed by fitting a delayed Gaussian to the leading edge of the initial descending limb of the ERG response at the top 2 luminous energies (1.20, 1.52 log c.s.m^-2) for each animal, based on the model of Lamb and Pugh²², formulated by Hood and Birch²³. This formula returns an amplitude and a sensitivity parameter, (Figure 1C and 1D, respectively). A hyperbolic function was fitted to the luminous energy response of rod bipolar cells for each animal, which also returned an amplitude and a sensitivity parameter, (Figure 1E and 1F respectively). Cone bipolar cell amplitude was analyzed as peak response of the waveform (top waveform of Figure 1A and 1B), with implicit time taken as the time it took to reach peak response. For further details please see Charng et al.²⁴.

Figure 1A and B shows ERG waveform ± SEMs (n = 8) in conscious rats at day 7 and 28 post-surgery. The waveforms appear to be slightly larger at day 28 compared to day 7, but linear mixed model analysis revealed no significant time effect (p = 0.14 to 0.67) for photoreceptor (dark-adapted PIII) amplitude (Figure 1C) and sensitivity (Figure 1D); rod bipolar cell (dark-adapted PII) amplitude (Figure 1E) and sensitivity (Figure 1F); cone bipolar cell (light-adapted PII) amplitude (Figure 1G) and implicit time (Figure 1H). Similarly, VEP waveform SEMs (n = 8, Figure 2A) appear comparable at 7 and 28 days post-surgery, with amplitude (Figure 2B and 2C) and timing (Figure 2D – 2F) parameters showing no significant time effect (p = 0.20 to 0.93). These results indicate robust ERG and VEP signal stability.

Average signal-to-noise (SNR, n = 8) ratio of both ERG (Figure 3A) and VEP (Figure 3B) returned good stability over the five conscious recording sessions. In this scenario, ERG signal is defined as the as the amplitude of the ERG P2 response while noise is the maximal peak to trough amplitude calculated from a 10 msec pre-stimulus interval. In the VEP, P2-N1 amplitude is deemed as the signal while noise is also returned by the peak to trough of the 10 msec pre-stimulus interval. There was no significant time effect across the SNR of both ERG and VEP (p = 0.49 and 0.62 respectively).

Figure 1: Conscious Electroretinograms Exhibit Characteristic Waveforms and Repeatable Measurements. (A–B) ERG waveforms ± SEMs (n = 8) across a wide range of luminous energies at day 7 (A) and 28 (B) post-surgery. (C-F) Rod and cone ERG parameters are plotted against time after implantation. Rod (dark-adapted PIII) photoreceptoral amplitude (C) and sensitivity (D), rod bipolar cell (dark-adapted PII) amplitude (E) and sensitivity (F), and cone bipolar cell (light-adapted PII) amplitude (G) and implicit time (H) all showed stable recordings over the 5 sessions. All symbols indicate average value (± SEM). This figure has been modified from Charng et al.²⁴ Figure 4. Please click here to view a larger version of this figure.

Figure 2: Conscious Visual Evoked Potentials Exhibit Characteristic Waveforms and Repeatable Measurements. (A) VEP waveforms ± SEMs (n = 8) are plotted at day 7 and 28 post surgery. (B–F) VEP amplitude and timing parameters are assessed over 1 month after implantation. P1-N1 (B) and P2-N1 (C) amplitude as well as P1 (D), N1 (E) and P2 (F) implicit time parameters were all stable over the 5 recording sessions. All symbols indicate average value (± SEM). This figure has been modified from Charng et al.²⁴ Figure 6. Please click here to view a larger version of this figure.

Figure 3: The Telemetry System Demonstrates Stable Signal-to-Noise Ratio Over Time. The signal-to-noise ratio of the (A) ERG and (B) VEP were not significantly altered over time (n = 8). All symbols indicate average value (± SEM). This figure has been modified from Charng et al.²⁴ Figure S1. Please click here to view a larger version of this figure.

Discussion

Due to the minimally invasive nature of visual electrophysiology, ERG and VEP recordings in human patients are conducted under conscious conditions and only require the use of topical anesthetics for electrode placement. In contrast, visual electrophysiology in animal models is conventionally conducted under general anesthesia to enable stable electrode placement by eliminating voluntary eye and body movements. However, commonly used general anesthetics alter the ERG and VEP responses as shown by our previous publication²⁴ and others^25-27. As such development of a conscious ERG and VEP platform in a rodent model provides superior representation of physiological responses in animal models, which may in turn afford better translatability from preclinical to clinical findings. Another disadvantage of using anesthesia is that it limits the duration of an experiment. More specifically, the use of prolonged anesthesia as well as repeated administration of anesthetics can increase chance of adverse effects such as drug build up and associated respiratory problems²⁸.

This study showed that the telemetry system in conscious rats returned robust ERG and VEP signal stability for at least 28 days post-surgery. Our group is the first to conduct conscious wireless ERG and VEP responses simultaneously²⁴ and this manuscript details the surgical and recording procedures involved. Comparison to other surgical procedures conducted with wired conscious ERG and VEP recordings illustrate superior stability in the ERG and equivalent repeatability in VEP recordings over a 1 month period¹⁵.

The surgical techniques and subsequent conscious recordings have the potential to be applied to various animal models. The platform has potential utility in multiple applications where it is beneficial to avoid confounds associated with anesthesia²⁹. These include drug discovery, improved translation to human studies, and chronic or longitudinal experiments.

Possible modifications to the technique include altering the number of biopotential channels implanted and simultaneously recorded. This can vary from 1 to 4 biopotential leads and thus could measure visual evoked electrophysiology from between 1 eye to 2 eyes and 2 visual cortices. Note that the alteration in the number of biopotentials channels also leads to modification of the band-width recorded which will have implications for high frequency electrophysiological signals. For example the 3 channel biopotential transmitter used in this study (F50-EEE) was chosen to show that it is possible to simultaneously record visually evoked responses from the retina and visual cortex of a conscious rat. However, these 3 channel transmitters have a band-width of 1 – 100 Hz, which can faithfully record ERG a- and b-waves but will alter oscillatory potentials due to their higher frequency²⁴. In contrast, if it was of interest to the study to record oscillatory potentials then a transmitter with less recording channels (i.e., broader band-width) could be employed. It is also possible for the light stimulus to be altered, for example instead of conducting full-field ERG and VEP, visual physiology in response to flicker stimuli may also be utilized.

One major limitation in translating this technique to other animal models is the size of the animal's eye. One should have no problem implanting the ocular electrodes to animals bigger than rats. However, it would be challenging to implant the ERG electrode onto a mouse eye due to the smaller working area. The cortical implantation, on the other hand, should be relatively straightforward to perform in most laboratory animals.

There are several aspects of the surgery that need to be closely observed to ensure successful implantation. It is imperative that the ERG electrode ring is formed into a smooth ring due to irritation that may be induced by any rough edges on the loop. The implantation of ERG active electrodes is facilitated by two concurrent experimenters, one to stabilize the eye while the other attaches the electrode to the sclera. Particular care has to be taken to ensure the scleral suture (2.2.19) is only half-thickness, as a full thickness scleral suture will puncture the eyeball and cause vitreous leakage. The implantation of electrodes onto the skull (VEP active and ERG/VEP inactive electrodes) is less technically demanding than that of ERG electrodes. Nevertheless, it is imperative that once the electrodes are anchored to the skull, the wires are allowed to uncurl naturally to reduce any unnecessary tension. Acclimatization to the recording restrainer prior to surgical implantation is advantageous to reduce excessive movements during ERG and VEP recordings.

Divulgations

The authors have nothing to disclose.

Acknowledgements

JC would like to acknowledge the David Hay Memorial Fund, The University of Melbourne for financial support in writing this manuscript. Funding for this project was provided by an ARC Linkage grant 100200129 (BVB, AJV, CTON).

Materials

Bioamplifier	ADInstruments	ML 135	Amplifies ERG and VEP signals
Carboxymethylcellulose sodium 1.0%	Allergan	CAS 0009000-11-7	Maintain corneal hydration during surgery
Carprofen 0.5%	Pfizer Animal Health Group	CAS 53716-49-7	Post-surgery analgesia, given with injectable saline for fluid replenishment
Chlorhexadine 0.5%	Orion Laboratories	27411, 80085	Disinfection of surgical instrument
Cyanoacrylate gel activator	RS components	473-439	Quickly dries cyanoacrylate gel
Cyanocrylate gel	RS components	473-423	Fix stainless screws to skull
Dental burr	Storz Instruments, Bausch and Lomb	E0824A	Miniature drill head of ~0.7mm diameter for making a small hole in the skull over each hemisphere to implant VEP screws
Drill	Bosch	Dremel 300 series	Automatic drill for trepanning
Enrofloxin	Troy Laboratories		Prophylactic antibiotic post surgey
Ganzfeld integrating sphere	Photometric Solutions International		Custom designed light stimulator: 36 mm diameter, 13 cm aperture size
Gauze swabs	Multigate Medical Products Pty Ltd	57-100B	Dries surgical incision and exposed skull surface during surgery
Isoflurane 99.9%	Abbott Australasia Pty Ltd	CAS 26675-46-7	Proprietory Name: Isoflo(TM) Inhalation anaaesthetic. Pharmaceutical-grade inhalation anesthetic mixed with oxygen gas for VEP electrode implant surgery
Kenacomb ointment	Aspen Pharma Pty Ltd		To reduce skin irritation and itching after surgery
Luxeon LEDs	Phillips Lighting Co.		For light stimulation, twenty 5 watt and one 1 watt LEDs, controlled by Scope software
Needle (macrosurgery)	World Precision Instruments	501959	for suturing abdominal and head surgery, used with 3-0 suture, eye needle, cutting edge 5/16 circle Size 1, 15mm
Needle holder (macrosurgery)	World Precision Instruments	500224	To hold needle during abdominal and head surgery
Needle holder (microsurgery)	World Precision Instruments	555419NT	To hold needle during ocular surgery
Optiva catheter	Smiths Medical International LTD	16 or 21 G	Guide corneal active electrodes from skull to conjunctiva
Povidone iodine 10%	Sanofi-Aventis	CAS 25655-41-8	Proprietory name: Betadine, Antiseptic to prepare the shaved skin for surgery 10%, 500 mL
Powerlab data acquisition system	ADInstruments	ML 785	Acquire signal from telemetry transmitter, paired to telemetry data converter
Proxymetacaine 0.5%	Alcon Laboratories	CAS 5875-06-9	Topical ocular analgesia
Restrainer	cutom made		Front of the restrainer is tapered to minimize head movement, length can be adjusted to accommodate different rat length, overall diameter is 60 mm.
Scapel blade	R.G. Medical Supplies	SNSM0206	For surgical incision
Scissors (macrosurgery)	World Precision Instruments	501225	for cutting tissue on the abodmen and forhead
Scissors (microsurgery)	World Precision Instruments	501232	To dissect the conjunctiva for electrode attachment
Scope Software	ADInstruments	version 3.7.6	Simultaneously triggers the stimulus via the ADI Powerlab system and collects data
Shaver	Oster	Golden A5	Shave fur from surgical areas
Stainless streel screws	MicroFasteners	L001.003CS304	0.7 mm shaft diameter, 3 mm in length
Stereotaxic frame	David Kopf	Model 900	A small animal stereotaxic instrument for locating the implantation landmarks on the skull
Surgical drape	Vital Medical Supplies	GM29-612EE	Ensure sterile enviornment during surgery
Suture (macrosurgery)	Ninbo medical needles	3-0	for suturing abdominal and head surgery, sterile silk braided, 60cm
Suture needle (microsurgery)	Ninbo medical needles	8-0 or 9-0	for ocular surgery including, suturing electrode to sclera and closing conjunctival wound, nylon suture, 3/8 circle 1×5, 30cm
Telemetry data converter	DataSciences International	R08	allows telemetry signal to interface with data collection software
Telemetry Data Exchange Matrix	DataSciences International		Gathers data from transmitters, pair with receiver
Telemetry data receiver	DataSciences International	RPC-1	Receives telemetry data from transmitter
Telemetry transmitter	DataSciences International	F50-EEE	3 channel telemetry transmitter
Tropicamide 0.5%	Alcon Laboratories		Iris dilation
Tweezers (macrosurgery)	World Precision Instruments	500092	Manipulate tissues during abdominal and head surgery
Tweezers (microsurgery)	World Precision Instruments	500342	Manipulate tissues during ocular surgery

References

Frishman, L. J. . Origins of the Electroretinogram. , (2006).
Granit, R. The components of the retinal action potential in mammals and their relation to the discharge in the optic nerve. J Physiol. 77, 207-239 (1933).
Brown, K. T. The eclectroretinogram: its components and their origins. Vision Res. 8, 633-677 (1968).
Brown, K. T., Murakami, M. Biphasic Form of the Early Receptor Potential of the Monkey Retina. Nature. 204, 739-740 (1964).
Kline, R. P., Ripps, H., Dowling, J. E. Generation of b-wave currents in the skate retina. Proc Natl Acad Sci U S A. 75, 5727-5731 (1978).
Krasowski, M. D., et al. Propofol and other intravenous anesthetics have sites of action on the gamma-aminobutyric acid type A receptor distinct from that for isoflurane. Mol Pharmacol. 53, 530-538 (1998).
Stockton, R. A., Slaughter, M. M. B-wave of the electroretinogram. A reflection of ON bipolar cell activity. J Gen Physiol. 93, 101-122 (1989).
Nixon, P. J., Bui, B. V., Armitage, J. A., Vingrys, A. J. The contribution of cone responses to rat electroretinograms. Clin Experiment Ophthalmol. 29, 193-196 (2001).
Weinstein, G. W., Odom, J. V., Cavender, S. Visually evoked potentials and electroretinography in neurologic evaluation. Neurol Clin. 9, 225-242 (1991).
Sand, T., Kvaloy, M. B., Wader, T., Hovdal, H. Evoked potential tests in clinical diagnosis. Tidsskr Nor Laegeforen. 133, 960-965 (2013).
Brankack, J., Schober, W., Klingberg, F. Different laminar distribution of flash evoked potentials in cortical areas 17 and 18 b of freely moving rats. J Hirnforsch. 31, 525-533 (1990).
Creel, D., Dustman, R. E., Beck, E. C. Intensity of flash illumination and the visually evoked potential of rats, guinea pigs and cats. Vision Res. 14, 725-729 (1974).
Herr, D. W., Boyes, W. K., Dyer, R. S. Rat flash-evoked potential peak N160 amplitude: modulation by relative flash intensity. Physiol Behav. 49, 355-365 (1991).
Guarino, I., Loizzo, S., Lopez, L., Fadda, A., Loizzo, A. A chronic implant to record electroretinogram, visual evoked potentials and oscillatory potentials in awake, freely moving rats for pharmacological studies. Neural Plast. 11, 241-250 (2004).
Szabo-Salfay, O., et al. The electroretinogram and visual evoked potential of freely moving rats. Brain Res Bull. 56, 7-14 (2001).
Valjakka, A. The reflection of retinal light response information onto the superior colliculus in the rat. Graefes Arch Clin Exp Ophthalmol. 245, 1199-1210 (2007).
Lapray, D., Bergeler, J., Dupont, E., Thews, O., Luhmann, H. J. A novel miniature telemetric system for recording EEG activity in freely moving rats. J Neurosci Methods. 168, 119-126 (2008).
Lim, K., Burke, S. L., Armitage, J. A., Head, G. A. Comparison of blood pressure and sympathetic activity of rabbits in their home cage and the laboratory environment. Exp Physiol. 97, 1263-1271 (2012).
Nguyen, C. T., Brain, P., Ivarsson, M. Comparing activity analyses for improved accuracy and sensitivity of drug detection. J Neurosci Methods. 204, 374-378 (2012).
Ivarsson, M., Paterson, L. M., Hutson, P. H. Antidepressants and REM sleep in Wistar-Kyoto and Sprague-Dawley rats. Eur J Pharmacol. 522, 63-71 (2005).
He, Z., Bui, B. V., Vingrys, A. J. The rate of functional recovery from acute IOP elevation. Invest Ophthalmol Vis Sci. 47, 4872-4880 (2006).
Lamb, T. D., Pugh, E. N. A quantitative account of the activation steps involved in phototransduction in amphibian photoreceptors. J Physiol. 449, 719-758 (1992).
Hood, D. C., Birch, D. G. Rod phototransduction in retinitis pigmentosa: estimation and interpretation of parameters derived from the rod a-wave. Invest Ophthalmol Vis Sci. 35, 2948-2961 (1994).
Charng, J., et al. Conscious wireless electroretinogram and visual evoked potentials in rats. PLoS Onez. 8, e74172 (2013).
Galambos, R., Szabo-Salfay, O., Szatmari, E., Szilagyi, N., Juhasz, G. Sleep modifies retinal ganglion cell responses in the normal rat. Proc Natl Acad Sci U S A. 98, 2083-2088 (2001).
Meeren, H. K., Van Luijtelaar, E. L., Coenen, A. M. Cortical and thalamic visual evoked potentials during sleep-wake states and spike-wave discharges in the rat. Electroencephalogr Clin Neurophysiol. 108, 306-319 (1998).
Nair, G., et al. Effects of common anesthetics on eye movement and electroretinogram. Doc Ophthalmol. 122, 163-176 (2011).
Amouzadeh, H. R., Sangiah, S., Qualls, C. W., Cowell, R. L., Mauromoustakos, A. Xylazine-induced pulmonary edema in rats. Toxicol Appl Pharmacol. 108, 417-427 (1991).
Charng, J., et al. Retinal electrophysiology is a viable preclinical biomarker for drug penetrance into the central nervous system. J Ophthalmol. , (2016).

Play Video

PDF

DOI

DOWNLOAD MATERIALS LIST

Citer Cet Article

Charng, J., He, Z., Bui, B., Vingrys, A., Ivarsson, M., Fish, R., Gurrell, R., Nguyen, C. Implantation and Recording of Wireless Electroretinogram and Visual Evoked Potential in Conscious Rats. J. Vis. Exp. (112), e54160, doi:10.3791/54160 (2016).