Primary Microglia Isolation from Postnatal Mouse Brains

Summary

Primary cell culture is one of the primarily used approaches for studying microglial biology in vitro. Here, we developed a method for simple and rapid microglia isolation from the mouse postnatal day 1 (P1) to P4.

Abstract

Microglia are the mononuclear phagocytes in the central nervous system (CNS), which play key roles in maintaining homeostasis and regulating the inflammatory process in the CNS. To study the microglial biology in vitro, primary microglia show great advantages compared to immortalized microglial cell lines. However, microglia isolation from the postnatal mouse brain is relatively less efficient and time-consuming. In this protocol, we provide a quick and easy-to-follow method to isolate primary microglia from the neonatal mouse brain. The overall steps of this protocol include brain dissection, primary brain cell culture, and microglia isolation. Using this approach, researchers can obtain primary microglia with high purity. In addition, the harvested primary microglia were able to respond to the lipopolysaccharides challenge, indicating they retained their immune function. Collectively, we developed a simplified approach to efficiently isolate primary microglia with high purity, which facilitates a wide range of microglial biology investigations in vitro.

Introduction

Microglia, the resident immune cells in the central nervous system (CNS), play pivotal roles in the maintenance of homeostasis, which respond to the neuropathological challenges¹. Recently, intensive investigations have been conducted to figure out the physiological functions of microglia, e.g., in Alzheimer's disease². Currently, the transcriptional profile of microglia at the single-cell resolution obtained during the CNS development, aging, and disease provides a better understanding of microglial function in healthy and diseased brains³. Previous studies identified a disease-associated microglial subtype in AD and other neurodegenerative diseases^4,5,6. This sub-population is proximal to the amyloid β (Aβ) deposition. Genes associated with phagocytosis and lipid metabolism (e.g., Apoe, Tyrobp) were found to be up-regulated in these populations^6,7. However, the subcellular processes, extracellular and intracellular signaling pathways that regulate the dynamic molecular profile changes in microglia are not fully understood. Particularly, the mechanism underlying chronic microglial activation in neurodegenerative diseases remains elusive. Therefore, it is crucial to understand microglia-involved cellular mechanisms since microglia responses clearly contribute to brain development and the progression of neurodegeneration.

Although there are a couple of in vivo and in vitro tools to study microglia, there are still some limitations. It is technically difficult to obtain a large enough number of microglial cells with high purity for routinely carrying out experiments, such as western blot, to elucidate intracellular signaling pathways. Primary microglia culture provides an alternative means to study the biology of microglia. The cultured primary microglia can be applied to analyze microglial phagocytic capacity after gene manipulation, and evaluate pro- and anti-inflammatory cytokines production in response to inflammatory stimuli, and other biological aspects to understand their roles in the brain⁸. Here, we present a new protocol and describe a step-by-step instruction for the isolation and culture of primary microglia from neonatal mouse brain, with emphasis on the steps that are critical for obtaining healthy and pure primary microglial cells.

Protocol

All the animal procedures were approved by the committee on Animal Research and the Institutional administration panel of laboratory animal care at Shanghai Jiao Tong University. Every effort has been made to minimize animal suffering.

1. Preparation of culture buffer, flasks, and coverslips

1. Culture medium and microglia culture medium: Supplement DMEM with 10% FBS to make the culture medium. The microglia culture medium is made by adding 10% FBS and 20% LADMAC conditioned medium to the DMEM. Add 1% Penicillin/Streptomycin to both the medium.
   1. To prepare 20% LADMAC conditioned medium, collect the culture medium from the LADMAC cells, centrifuge at 200 x g for 10 min, filter using 0.22 µm cell strainer, and then store the aliquots at -80 °C.
2. Digestion buffer: Prepare digestion buffer by adding 8 U/mL papain and 125 U/mL DNase to DMEM.
   NOTE: For best results, the digestion buffer should be prepared freshly. Calculate the desired amount based on the number of pups (1 mL solution for every 2 pups).
3. Coating flasks: Use T25 or T75 flasks for pre-plating the isolated brain cells. Before the brain dissection, coat T25 flasks with 2 mL (or 4 mL for a T75 flask) of 0.1 mg/mL Poly-D-lysine (PDL) and incubate at 37 °C for at least 1 h. Aspirate the PDL solution, wash twice with 1x PBS, and then allow the flask to air-dry in the cell culture hood.
   NOTE: The size and number of flasks used in the experiment were dependent on the number of postnatal pups. To let the cells reach the confluent astrocyte cell layer in a short time, prepare one T25 flask for 3-5 brains, or one T75 flask for 5 brains. Unused coated flasks can be stored at 4 °C for up to a month. To save time, 10x (1 mg/mL) stock solution of PDL can be prepared before the start of the experiment and stored at -20 °C as single-use aliquots. Dilute the aliquots in sterile 1x PBS right before use.
4. Prepare coverslips: Wash commercial glass coverslips with 0.1 M HCl for 1 h, rinse twice with autoclave water, then store in 100% ethanol. Before use, flame the coverslips using fine forceps with a burner lamp to remove residual ethanol. 8 mm glass coverslips can be placed in a 48-well plate, and 12 mm glass coverslips can be placed in a 24-well plate.
5. Prepare dissection tools: Soak fine scissors, forceps, and stainless steel micro-spoons in 75% ethanol for at least 20 min. Then place these tools under ultraviolet radiation in the tissue culture hood for 30 min.

2. Dissection of mouse brain

NOTE: To evaluate the efficacy of the protocol, here we used CX3CR1^GFP knock-in mice for tracing microglia⁹. CX3CR1^GFP/GFP mice and wild type C57BL/6J females at 2- to 8-month were crossed to generate CX3CR1^+/GFP mice, both were originally obtained from commercial sources. Mice were housed under a 12-12 h light-dark cycle in a specific pathogen-free (SPF) environment at Shanghai Jiao Tong University. Pups from postnatal day 1 to day 4 can be used for this protocol.

1. Decapitate all pups with surgical scissors. To minimize contamination, rinse all heads with 75% ethanol and quickly put in the ice-cold 1x PBS. Meanwhile, warm the digestion buffer and co-culture medium in a 37 °C water bath.
   NOTE: Decapitate and isolate brain tissue from one pup at a time to preserve structural integrity. To prevent contamination, all surgical tools should be placed in 75% ethanol between decapitation.
2. Use fine dissecting scissors to cut the skull along with the medulla oblongata. Place a stainless steel micro-spoon beneath the brain tissue from the cutting site to squeeze out the brain from the head cavity. Transfer it to a new chilled 6-well plate containing 2 mL of pre-cold 1x PBS per well.
3. Cut off and discard the cerebellum and olfactory bulbs. Gently transfer the remaining brain tissue to a chilled 6-well plate containing 2 mL of pre-cold 1x PBS.
   NOTE: Place 4-5 brain tissues in one well.
4. Repeat the same procedure for the remaining heads until all tissue is collected.

3. Seed the mixed primary cells

1. Aspirate 1.5 mL of 1x PBS in the 6-well plate, and fully mince the brain tissue into small pieces (approximate 1 mm²) with the help of spring scissors.
   NOTE: To reduce the amount of fine debris, do not over mince the tissue.
2. Add the desired amount of digestion buffer to the well (0.5 mL of digestion buffer per brain), then place the plate in the 5% CO₂, 37 °C humidified incubator for 20 min. Swirl the plate every 10 min.
   NOTE: During the incubation time, wet a 70 µm cell strainer with culture medium (10% FBS in DMEM), and then place the cell strainer onto a fresh 50 mL collection tube.
3. Take the plate out of the incubator and terminate papain digestion by adding 3 mL of culture medium to each well. Mildly pipette the cells up and down 10 times using a 1 mL pipette. Transfer the mixture to a 15 mL tube, and let it settle for 1 min. A cloudy cell pellet can be seen at the bottom. To remove big clumps and cell debris, carefully pass the cell suspension through a 70 µm cell strainer and collect the flow-through in the 50 mL collection tube.
4. Add 3 mL of warmed culture medium (10% FBS in DMEM) to the undissociated cell pellet in the 15 mL tube. Triturate 10 times as in steps 3.3 to continue the dissociation. Let the tissue settle for 1 min and then pass the cell suspension through the strainer to the 50 mL collection tube. Repeat this step, and discard the remaining cell debris.
5. Transfer the cell suspension from the 50 mL collection tube to 15 mL tubes and centrifuge the cells at 200 x g for 10 min at room temperature.
6. Aspirate the supernatant, and resuspend the cells in 5 mL of culture medium. Seed the primary cells in a T25 or T75 flask at a cell density of about 5 x 10⁶ and culture in the humidified incubator (5% CO₂, 37 °C). This is Day 0 in this culture schedule.
   ​NOTE: If cells are seeded in a T25 flask, a final volume of 5 mL medium per flask is sufficient. Add an extra 5 mL of culture medium to each flask when seeded in a T75 flask.

4. Collection of primary microglia

1. Evaluate the confluency of the mixed cells on the next day (Day 1). Since the mixed cells were seeded at a pretty high density, it takes 3-4 days for the astrocytes to reach confluency, allowing the microglia to be collected 1-2 days later.
   NOTE: Be cautious if cells are not attached to the bottom of the flask on the next day; it might be due to cell contamination or cell death caused by over digestion or harsh handling.
2. On Day 2, wash the flasks with 3 mL of warm 1x PBS twice and change the medium by adding 3-5 mL of fresh culture medium to each T25 flask (7-10 mL for a T75 flask). The discarded culture medium contains cell debris and various types of cells, including neurons, oligodendrocytes and microglia.
3. On Day 4, ensure that astrocytes attached to the bottom of the flask are at 100% confluency. Meanwhile, a subpopulation of microglia is loosely attached to the mixed cell surface layer which can easily detach from the surface and float in the culture medium by handshaking. Transfer the culture medium to a fresh 6-well plate, and primary microglia enriched in the medium are collected during this process. Next, provide the cells on the original 6-well plate with fresh culture medium for further cell collection.
   NOTE: Tapping the flasks on the table or shaking the flasks on a laboratory shaker at 180 rpm for 30 min before medium transferring is appropriate to yield more cells.
4. Carefully place the 6-well to the incubator to allow cell attachment. About 2 h after incubation, all the cells will be attached to the plate. When the cells are attached, gently wash them with warm 1x PBS twice to remove cell aggregates and cell debris; then, supply the cells with 3 mL of fresh microglia culture medium. The isolated microglia cells can be maintained for more than a month in vitro by refreshing the microglia culture medium every 2 days.
   NOTE: Colony-stimulating factor 1 (CSF1) is an important growth factor to support microglia survival in vitro. Previous studies report that CSF1 can be secreted from the LADMAC cell line, which is a transformed cell line originated from mouse bone marrow cells. The LADMAC conditioned medium can be collected by centrifuging the LADMAC culture at 200 x g for 10 min; then, pass the supernatant through a 0.22 µm cell strainer. Microglia culture medium was prepared by adding 20% LADMAC conditioned medium to the culture medium (10% FBS, DMEM).
5. Every 2-3 days, continue to collect the microglia from the mixed cell culture medium as in step 4.4. Culture the remaining mixed cells in the flask and use them for consistently harvesting microglia every 2-3 days for up to 1 month.
   NOTE: Microglia can be successfully harvested by collecting the medium form mixed culture cells for up to 50 days. Each time, the collected co-culture medium will yield about ~1-3 x 10⁵ microglia cells per T75 flask. Combine microglial cells, if needed.
6. Use primary microglial cells for the desired functional assay.

Results

Primary microglia collected from CX3CR1^+/GFP at Day 7 and Day 35 after cell seeding were demonstrated in Figure 1. As shown in the immunofluorescence staining of microglia/macrophage cell marker IBA1, all IBA1 positive cells are positive for the GFP signals, and negative for S100β (astrocyte marker) and CC1(oligodendrocyte marker), suggesting that the purified GFP positive cells are indeed microglia. Next, it was found over 95% of isolated cells are GFP positive cells, i...

Discussion

This protocol is based on the methods described previously with some modifications¹¹. Tips for improving the viability and purity of isolated microglia are listed as follows. First, take care to avoid contamination when preparing buffers used for tissue isolation and cell culture. Make sure the surgery tools, containers, and plastic equipment are sterile. Usually, we perform the brain dissection in a separate tissue culture hood aside from the cell culture hood for general cell culture to avoid cr...

Materials

Name	Company	Catalog Number	Comments
Cell strainers, 40 µm	ThermoFisher Scientific	22-363-547
DNase I	Sigma	11284932001
Dulbecco's Modified Eagle Medium (DMEM)	Gibco by Life Technologies	C11995500BT
Dulbecco's Phosphate Buffered Saline (DPBS)	Gibco by Life Technologies	14190-144
Fetal Bovine Serum (FBS)	Gibco by Life Technologies	10099141
Papain, Suspension	Sangon Biotech	Papain, Suspension
Penicillin-Streptomycin 100X solution	Hyclone	SV30010
Poly-D-Lysine	ThermoFisher Scientific	A3890401