Demyelinating diseases can be modeled in animals by focal application of lysolecithin into the CNS. A single injection of lysolecithin into mouse spinal cord produces a lesion that spontaneously repairs over time. The goal is to study factors involved in de- and remyelination, and to test agents for enhancing repair.
Multiple sclerosis is an inflammatory demyelinating disease of the central nervous system characterized by plaque formation containing lost oligodendrocytes, myelin, axons, and neurons. Remyelination is an endogenous repair mechanism whereby new myelin is produced subsequent to proliferation, recruitment, and differentiation of oligodendrocyte precursor cells into myelin-forming oligodendrocytes, and is necessary to protect axons from further damage. Currently, all therapeutics for the treatment of multiple sclerosis target the aberrant immune component of the disease, which reduce inflammatory relapses but do not prevent progression to irreversible neurological decline. It is therefore imperative that remyelination-promoting strategies be developed which may delay disease progression and perhaps reverse neurological symptoms. Several animal models of demyelination exist, including experimental autoimmune encephalomyelitis and curprizone; however, there are limitations in their use for studying remyelination. A more robust approach is the focal injection of toxins into the central nervous system, including the detergent lysolecithin into the spinal cord white matter of rodents. In this protocol, we demonstrate that the surgical procedure involved in injecting lysolecithin into the ventral white matter of mice is fast, cost-effective, and requires no additional materials than those commercially available. This procedure is important not only for studying the normal events involved in the remyelination process, but also as a pre-clinical tool for screening candidate remyelination-promoting therapeutics.
Multiple sclerosis (MS) is a chronic demyelinating disease of the central nervous system (CNS) characterized by immune cell infiltration and plaques containing lost myelin, oligodendrocytes, axons and neurons. Most patients have a disease course consisting of inflammatory relapses accompanied by a wide range of neurological symptoms, followed by periods of remission. Over half of these patients eventually transition to a secondary progressive stage with no apparent relapses but continual neurological decline. It is believed that this progressive deterioration is due to axonal damage and loss, contributed in part by chronic demyelination. Strategies to restore lost myelin are thus considered a promising treatment approach to delay disease progression and perhaps reverse neurological symptoms.
Remyelination is an endogenous repair response in the CNS whereby new myelin sheaths are generated from recruited oligodendrocyte precursor cells (OPCs) that differentiate into myelin-forming oligodendrocytes. Remyelination has been shown in animal models to be quite robust1-3, however, its efficiency declines with age4. Indeed, remyelination occurs in humans although it is incomplete in the majority of MS patients5. All currently available medications for MS primarily target the aberrant immune component of the disease and, while effective at reducing relapses, do not markedly delay disease progression. The next generation of therapeutic strategies for the management of MS will integrate advances in immunomodulation with the enhancement of endogenous remyelination in order to prevent both relapses and progression6.
One method to study de- and remyelination in the CNS involves the direct injection of the detergent lysophosphatidylcholine (lysolecithin) into the spinal cord white matter1,3,7. This procedure produces a well characterized demyelinating injury consisting principally of macrophage/microglial infiltration and activation8,9, reactive astrogliosis, perturbation of axonal homeostasis/axonal injury, and OPC proliferation and migration10. The lesion predictably evolves over the period of a few weeks and is eventually capable of fully remyelinating. This method has been particularly useful in studying the choreography of events involved in de- and remyelination. Further, it has been adopted as a tool for pre-clinical testing of candidate therapies to accelerate repair following a demyelinating insult.
A number of animal models have been developed to study MS, most recognizably the experimental autoimmune encephalomyelitis (EAE) model. In EAE, rodents are immunized against a fragment of a myelin peptide and undergo inflammatory lesion development manifesting in ascending paralysis. While this model has been useful for pre-clinical testing of immunomodulatory MS drugs, it is not ideal for studying remyelination for three main reasons: Firstly, the location of inflammatory lesions is somewhat random, and locating lesions when processing tissue for semi- or ultrathin sections can be challenging. The second is that remyelination occurs over a specific time course, and the exact age of a single EAE lesion cannot be known without continual non-invasive magnetic resonance imaging. The third is that remyelination is a naturally occurring phenomenon in rodents, and evidence of remyelination following drug treatment in EAE may not be a primary result of the drug, but instead a secondary phenomenon of reducing inflammation.
Another common method of producing demyelination is achieved by introducing the copper chelator cuprizone in the diet. This results in widespread demyelination, most notably in the corpus callosum. There are limitations in studying the corpus callosum as a site of remyelination for the following reasons: Firstly, axon diameters (and thus myelin thickness) are smaller than other CNS regions, and thus thinly remyelinated sheaths can be indistinguishable from those that were never demyelinated. Secondly, because the mouse corpus callosum contains >70% unmyelinated axons16, it can be unclear whether a remyelinated segment is true repair of damaged myelin or de novo myelin synthesis in the adult, which occurs normally17.
It is of our belief that the best model for studying remyelination is the direct injection of toxins, either lysolecithin, ethidium bromide, or others, into the caudal cerebral peduncles18 or the spinal cord white matter. The former location is achieved only by precise 3-dimension stereotactic injection, and is limited to larger rodents (rats) due to the small size of the cerebellar peduncles. This excludes the extensive resource of transgenic mice in studying de- and remyelination. The spinal cord, however, contains many large white matter tracts that are easily accessible surgically. Spaces between vertebrae in the rostral thoracic segment allows for exposure of the spinal cord without the need for a laminectomy, which is a necessary step in caudal thoracic surgical procedures. An advantage of specifically targeting the ventral white matter is that the axons are uniformly larger than the dorsal white matter, making quantification of remyelination a less ambiguous task—similar to the challenges associated with the corpus callosum. Additionally, the ventral white matter makes up a much larger target area to inject; several hundred microns laterally in the dorsal region would place the capillary outside the column, while the same deviation ventrally would still produce a prominent demyelinating lesion. Some protocols inject lysolecithin into both the dorsal and ventral columns of the same animal19. This can increase both the likelihood of proper capillary placement and the number of quantifiable lesions in fewer animals. While the current data presented is from 8-10 week old animals at time of operation, we have also had success using the same procedure on 8-10 month old mice, where remyelination is described as being markedly slower4.
Quantification of remyelination is not a trivial undertaking. A central dogma posits that remyelinated segments are shorter in length and thinner on average than their healthy counterparts, and thus g-ratio calculations (axon diameter divided by axon + myelin diameter) of cross-sectional semi- or ultrathin sections have become standard procedure. However, it is known that remyelinated segments thicken over time2 and a recent study using a transgenic reporter of remyelinating oligodendrocytes suggests that many internodes eventually become indistinguishable from control20. Quantifying the number of mature oligodendrocytes within the lesion is an indirect way to measure repair, as oligodendrocytes are capable of making a wide number of internodes, and a significant proportion of remyelination—depending on the model used—can occur from Schwann cells3. Of course, as remyelination has been linked to restoration of saltatory conduction21, the ultimate metric of repair would be functional recovery of neurological deficits. While remyelination has been linked to recovery of function in some species22,23, it has not become a standard procedure in murine lysolecithin studies. This is likely due to a lack of overt observable deficits from either dorsal or ventral lesions, compared to more robust demyelination models such as EAE and even cuprizone. We believe that functional deficits resulting from lysolecithin injection, and subsequent recovery with remyelination, will only be observable using sensitive tests of fine sensorimotor functioning.
A PubMed search of “remyelination” alongside either of the animal models listed above, albeit a brusque methodological approach, shows fewer search hits for lysolecithin (109) compared to EAE (188) and cuprizone (197). If our argument that lysolecithin demyelination is the superior approach for studying remyelination, why is it the least discussed? Perhaps an apprehension for using this method derives from a belief of technical difficulty in performing the surgical operation. In actuality, this procedure is fast, cost-effective, and is no more difficult than routine tissue dissection, requiring materials that are all commercially available. It is our hope that this protocol proves useful for those that wish to add this powerful model to their repertoire for studying the exciting and expanding field of myelin repair.
The authors have nothing to disclose.
This project was funded by a grant from the Multiple Sclerosis Society of Canada and the Alberta Innovates – Health Solutions CRIO Team program. MBK is a recipient of studentships from Alberta Innovates – Health Solutions and the Multiple Sclerosis Society of Canada. SKJ is funded by a graduate student support grant from the Alberta endMS Regional Research and Training Center of the Multiple Sclerosis Society of Canada. The authors wish to acknowledge Dr. Jan van Minnen and the Regeneration Unit in Neurobiology core facility for training and use of equipment.
Name of Material/ Equipment | Company | Catalog Number | Comments/Description |
spring scissors | Fine Science Tools | 15004-08 | |
forceps | Fine Science Tools | 11254-20 | |
retractor | Fine Science Tools | 17003-03 | |
clippers | Philips | QG3330 | |
heating recovery chamber | Peco Services | V1200 | |
surgical tape | 3M | 1527-1 | |
scalpel handle | Fine Science Tools | 10003-12 | |
scalpel blade | Feather | No. 15 | |
sponge spear | Beaver Visitec | 581089 | |
5-0 Vicryl sutures | Ethicon | J511G | |
curved ToughCut spring scissors | Fine Science Tools | 15123-12 | |
32 gauge metal needle | BD | 305106 | |
needle holders | Fine Science Tools | 12002-14 | |
angled forceps | Fine Science Tools | 11251-35 | |
cotton tipped applicator | Puritan | 806-WC | |
gauze pads | Safe Cross First Aid | 3763 | |
10 μL syringe | Hamilton | 7635-01 | make sure to purchase the microliter, not gastight syringe |
compression fitting | Hamilton | 55750-01 | contains the 2 ferrules and removable nut, but the nut that comes with the 10 μL syringe is a tighter fit |
priming kit | Hamilton | PRMKIT | contains the priming syringe, removable hub needle and the rubber discs |
pre-pulled glass capillaries | WPI | TIP10TW1 (pack of 10) | contains capillaries with 10 μm inner diameter. 30 μm inner diameter also work (TIP30TW1) |
stereotactic frame | David Kopf instruments | Model 900 | |
Ultrasonic cleaner | Fisher Scientific | FS-20 | |
Tissue-Tek optimal cutting temperature (OCT) compound | VWR | 25608-930 | |
Tissue-Tek intermediate cryomold | VWR | 25608-924 | |
cryostat | Leica | CM1900 | |
microscope slides | VWR | 48311-703 | |
bright field microscope | Olympus | BX51 | |
ultramicrotome | Leica EM UC7 | EM UC7 | |
Lysophosphatidylchoine | Sigma | L1381 | |
2-methylbutane | Sigma | M32631 | |
Triton x-100 | Sigma | X-100 | |
goat serum | Sigma | G9023 | |
Mouse anti-SMI312 antibody | Covance | SMI-312R | 1:2000 dilution |
Rabbit anti-MBP antibody | Abcam | AB40390 | 1:1000 dilution |
Goat anti-PDGFRα antibody | R&D Systems | AF1062 | 1:100 dilution |
Rabbit anti-Olig2 antibody | Millipore | AB9610 | 1:200 dilution |
Mouse anti-CC1 antibody | Calbiochem | OP80 | 1:200 dilution |
Alexa Fluor 488 goat anti-rabbit IgG | Life technologies | A-11008 | 1:500 dilution |
Alexa Fluor 546 goat anti-mouse IgG | Life technologies | A-11003 | 1:500 dilution |
Alexa Fluor 488 donkey anti-goat IgG | Jackson Immuno | 705-546-147 | 1:500 dilution |
Alexa Fluor 594 donkey anti-mouse IgG | Jackson Immuno | 715-586-151 | 1:500 dilution |
Alexa Fluor 647 donkey anti-rabbit IgG | Jackson Immuno | 711-606-152 | 1:500 dilution |
PBS | Oxoid | BR0014 | |
isopropyl alcohol | Sigma | 109827 | |
ketamine | CDMV | ||
xylazine | CDMV | ||
iodine | West Penetone | 2021 | |
Vaseline petroleum jelly | VWR | CA05971 | |
paraformaldehyde | Sigma | P6148 | |
sucrose | Sigma | S5016 | |
Eriochrome Cyanine R | Sigma | 32752 | |
sulfuric acid | Sigma | 320501 | |
iron(III) chloride | Sigma | 157740 | |
ammonium hydroxide | Sigma | 320145 | |
Acrytol | Leica Biosystems | 3801700 | |
Citrisolv | Fisher Scientific | 22-143-975 | |
horse serum | Sigma | H0146 | |
glutaraldehyde | Electron Micrscopy Sciences | 16220 | |
osmum tetroxide | Electron Micrscopy Sciences | 19150 | highly toxic |
potassium hexacyanoferrate (II) trihydrate | Sigma | P3289 | |
corn oil | Sigma | C8267 | |
polyvinyl alcohol | Sigma | P8136 | |
glycerol | Sigma | G9012 | |
cacodylic acid | Electron Micrscopy Sciences | 12300 | |
propylene oxide | Electron Micrscopy Sciences | 20401 | |
EMBED kit | Electron Micrscopy Sciences | 14120 | |
Toluidine Blue O | Sigma | T3260 | |
Sodium tetraborate decahydrate | Sigma | S9640 | |
Recipes | |||
Eriochrome cyanine solution | |||
Ingredient | Amount to add | ||
Eriochrome Cyanine R | 0.8 g | ||
sulfuric acid | 400 mL 0.5% | ||
iron(III)chloride | 20 mL 10% | ||
water | 80 mL | ||
*add eriochrome cyanine to sulfuric acid, followed by iron(III) chloride and water. Solution can be kept after use. Make fresh once per year. | |||
Gelvatol | |||
Ingredient | Amount to add | ||
PBS | 140 mL | ||
polyvinyl alcohol | 20 g | ||
glycerol | 40 g | ||
*mix well, place at 37 °C overnight, centrifuge at 1960xg 30 min, aliquot into 40 tubes |