Isolation and Identification of Mesenchymal Stem Cells Derived from Adipose Tissue of Sprague Dawley Rats

Summary

This protocol describes a methodology for isolating and identifying adipose tissue-derived mesenchymal stem cells (MSCs) from Sprague Dawley rats.

Abstract

Adult mesenchymal cells have revolutionized molecular and cell biology in recent decades. They can differentiate into different specialized cell types, in addition to their great capacity for self-renewal, migration, and proliferation. Adipose tissue is one of the least invasive and most accessible sources of mesenchymal cells. It has also been reported to have higher yields compared to other sources, as well as superior immunomodulatory properties. Recently, different procedures for obtaining adult mesenchymal cells from different tissue sources and animal species have been published. After evaluating the criteria of some authors, we standardized a methodology that is applicable to different purposes and easily reproducible. A pool of stromal vascular fraction (SVF) from perirenal and epididymal adipose tissue allowed us to develop primary cultures with optimal morphology and functionality. The cells were observed adhered to the plastic surface for 24 h, and exhibited a fibroblast-like morphology, with prolongations and a tendency to form colonies. Flow cytometry (FC) and immunofluorescence (IF) techniques were used to assess the expression of the membrane markers CD105, CD9, CD63, CD31, and CD34. The ability of adipose-derived stem cells (ASCs) to differentiate into the adipogenic lineage was also assessed using a cocktail of factors (4 µM insulin, 0.5 mM 3-methyl-iso-butyl-xanthine, and 1 µM dexamethasone). After 48 h, a gradual loss of fibroblastoid morphology was observed, and at 12 days, the presence of lipid droplets positive to oil red staining was confirmed. In summary, a procedure is proposed to obtain optimal and functional ASC cultures for application in regenerative medicine.

Introduction

Mesenchymal stem cells (MSCs) have strongly impacted regenerative medicine due to their high capacity for self-renewal, proliferation, migration, and differentiation into different cell lineages^1,2. Currently, a great deal of research is focusing on their potential for the treatment and diagnosis of various diseases.

There are different sources of mesenchymal cells: bone marrow, skeletal muscle, amniotic fluid, hair follicles, placenta, and adipose tissue, among others. They are obtained from different species, including humans, mice, rats, dogs, and horses³. Bone marrow-derived MSCs (BMSCs) have been used for many years as a major source of stem cells in regenerative medicine and as an alternative to the use of embryonic stem cells⁴. However, adipose-derived MSCs, or adipose-derived stem cells (ASCs), are an important alternative with great advantages due to their ease of collection and isolation, as well as the yield of cells obtained per gram of adipose tissue^5,6. It has been reported that the harvest rate of ASCs is generally higher than that of BMSCs⁷. It was initially proposed that the reparative/regenerative capacity of ASCs was due to their ability to differentiate into other cell lineages⁸. However, research in recent years has reinforced the primary role of paracrine factors released by ASCs in their reparative potential^9,10.

Adipose tissue (AT), in addition to being an energy reserve, interacts with the endocrine, nervous, and cardiovascular systems. It is also involved in postnatal growth and development, the maintenance of tissue homeostasis, tissue repair, and regeneration. The AT is composed of adipocytes, vascular smooth muscle cells, endothelial cells, fibroblasts, monocytes, macrophages, lymphocytes, preadipocytes, and ASCs. The latter possess an important role in regenerative medicine due to their low immunogenicity^11,12. ASCs can be obtained by enzymatic digestion and mechanical processing or by adipose tissue explants. Primary cultures of ASCs are easy to maintain, grow, and expand. Phenotypic characterization of ASCs is essential to verify the identity of the cells by assessing the expression of specific membrane markers using methods such as immunofluorescence and flow cytometry¹³. The International Federation for Adipose Therapeutics and Science (IFATS) and the International Society for Cellular Therapy (ISCT) have defined that ASCs express CD73, CD90, and CD105, while lacking the expression of CD11b, CD14, CD19, CD45, and HLA-DR¹⁴. These markers, both positive and negative, are therefore considered reliable for the characterization of ASCs.

This project was focused on describing a procedure for the isolation and identification of adult mesenchymal cells extracted from rats’ AT, as this source of cells does not present ethical challenges, unlike embryonic stem cells. This solidifies the procedure as a viable option because of the ease of access and minimally invasive method compared to bone marrow-derived stem cells.

Mesenchymal cells from this tissue source have an important role in regenerative medicine because of their immunomodulatory capabilities and low immune rejection. Therefore, the present study is a fundamental part of future research into their secretome and their application as regenerative therapy in different diseases, including metabolic diseases such as diabetes.

Protocol

All experimental procedures were performed following Mexican Guidelines for Animal Care, based on recommendations of the Association for Assessment and Accreditation of Laboratory Animal Care International (Norma Oficial Mexicana NOM-062-200-1999, Mexico). The protocol was reviewed, approved, and registered by the Ethics Committee for Health Research of the Instituto Mexicano del Seguro Social (R-2021-785-092).

1. Removal of adipose tissue from rats by surgical resection

1. Prepare two conical tubes with 20 mL of sterile 1x phosphate buffered saline-antibiotic antimycotic (PBS-AA) solution (1x PBS, gentamicin [20 µg/mL], and amphotericin [0.5 µg/mL]) and maintain on ice.
2. Select two adult male Sprague Dawley rats (R. norvegicus) in good health condition. Ensure the rats are between 3-4 months old and have a coporal weight of 350-450 g.
3. Proceed to sedation with 20 mg/kg xylazine hydrochloride, and 5 minutes later, administer an anesthetic with a dose of 120 mg/kg ketamine hydrochloride intraperitoneally. Lubricate both eyes with an ophthalmic ointment to prevent drying. Then, confirm anesthesia depth via lack of pedal reflex. 
4. Shave and disinfect the abdominal and inguinal region with an iodine solution. Apply surgical drapes to maintain sterility. Then, make a median longitudinal incision from the sternum to the testicular region.
5. Remove the adipose tissue surrounding both the epididymis and the kidneys with sterile forceps and place in the 1x PBS-AA solution. Keep the samples on ice.
6. Suture the incision closed if requires per the institutional guidelines and euthanize the animals with an intracardiac dose of 40 mg/kg sodium pentobarbital. Once death is confirmed, dispose the carcass following institutional procedure(s).
   NOTE: Death elicits signaling mechanisms that affect immunophenotype, differentiation capacity, and paracrine effect of mesenchymal cells. Hence, tissue collection is performed before euthanasia. 

2. Isolation of mesenchymal cells from adipose tissue

1. Remove the adipose tissue with sterile forceps within a biosafety cabinet and place it on sterile filter paper in a 100 mm diameter Petri dish to absorb excess PBS.
2. Transfer the adipose tissue to another Petri dish and perform three washes for 5 min each with 10 mL of 1x PBS-AA solution using a 10 mL pipette.
3. Mechanically disaggregate the tissue into fragments of approximately 1 cm² using scissors and a scalpel.
4. Prepare collagenase type IV (0.075%) in 20 mL of non-supplemented Dulbecco's modified Eagle's medium (DMEM). Filter through a 0.22 µm syringe filter and keep at 37 °C.
5. Add the collagenase solution (20 mL) prepared in step 2.4 into a crystal beaker with the fragmented tissue and a magnetic bar. Seal the container and incubate under slow and continuous agitation at 37 °C.
   NOTE: The enzymatic digestion takes approximately 90 min (maintain slow stirring to preserve the integrity of the cell membranes).
6. Filter the homogenate through a stainless steel, 40 mesh, 0.38 mm aperture filter on a 100 mm Petri dish and collect the cell suspension in a sterile 50 mL conical tube.
7. Add 20 mL of warmed, supplemented DMEM (10% fetal bovine serum [FBS], 2 mM glutamine, 2 mM sodium pyruvate, 100x non-essential amino acid solution, and 100x antibiotic antimycotic solution [AA]). Carefully suspend the stromal vascular fraction (SVE).
8. Centrifuge the cell suspension at 290 x g for 10 min, discard the supernatant with a 25 mL pipette, and gently wash the cells with 40 mL of a non-supplemented DMEM medium.
9. Repeat this step. Use a new sterile conical tube between steps to drag the least amount of cellular detritus and fat.
10. Suspend the pellet in 5 mL of supplemented DMEM with a 5 mL pipette and transfer to a T-25 cm² bottle. Incubate for 24 h at 37 °C and 5% CO₂.
11. The following day, perform three washes with 5 mL of warmed 1x PBS-AA and two washes with non-supplemented DMEM to remove cell debris and non-adherent cells. Add 5 mL of fresh, warmed, supplemented DMEM with a 5 mL pipette and change the medium every 3-4 days.

3. Maintaining and expansion of the ASC primary cultures

1. Once the cells reach 90%-100% confluence (8 ± 2 days), wash twice with 5 mL of non-supplemented DMEM. Add 1 mL of warmed 0.025% Trypsin-2 mM Ethylenediaminetetraacetic acid (EDTA) and incubate for 5-7 min at 37 °C.
2. When the cell monolayer is detached, add 4 mL of supplemented DMEM and gently disaggregate the cell suspension.
3. Transfer the cell suspension to a 15 mL conical tube, add 5 mL of warmed, supplemented DMEM, and gently suspend to homogenize.
4. Centrifuge at 290 x g for 5 min. Discard the supernatant and gently mix the pellet in 1 mL of supplemented DMEM. Count the cells in a Neubauer chamber after staining with Trypan blue.
5. Finally, seed 2.5 x 10³ cells/cm² at a split ratio of 1:4 in T-75 flasks. This step ensures colony formation and a high proliferation rate.

4. Morphology characterization of ASC primary cultures

1. Observe the morphology of ASCs under inverted microscopy.
   NOTE: Before mounting for histology and ASC identification, treat the coverslips with a 1% gelatin solution. Irradiate with UV for 15 min.
   1. Remove the coverslips from the 70% ethanol solution and allow them to dry for 5 min.
   2. Immerse the coverslips in a sterile 1% gelatin solution, drain, and dry at room temperature (RT).
   3. Place each coverslip into each well of a 6-well plate and irradiate the plates with UV light for 15 min.
   4. Seed a drop containing 25 x 10³ cells in the center of the well, wait 1 min, and add 1 mL of supplemented DMEM medium. Incubate for 96 h at 37 °C and 5% CO₂.
   5. Remove the medium and perform three washes with 1x PBS-AA using a transfer pipette.
   6. Add 1 mL of 3.5% neutral formalin to each well and incubate for 1 h at RT. Carefully remove the formalin and add 1 mL of cold 70% ethanol to each well.
   7. Seal the plate with parafilm until use, to prevent drying out.
      NOTE: The cellular morphology of ASCs are also evaluated by hematoxylin-eosin staining during different passages.
   8. Remove the 70% ethanol from each well and hydrate the cells for 5 min with distilled water. Meanwhile, filter the staining solutions.
   9. Remove the water and stain the cells under slow agitation for 15 min with Harris' hematoxylin solution.
   10. Remove the staining solution and perform two washes with 1x PBS.
   11. Stain the cells with eosin solution under slow agitation for 1 min. Then, remove the solution and perform two washes with 1x PBS.
   12. Carefully remove the coverslips from each well and mount the slides on a drop of PBS-glycerol mounting solution (1:1 v/v).
   13. Place a line of nail varnish around the coverslip and observe the histological slides under the light microscope.

5. Expression markers of ASCs by immunofluorescence

1. Prepare the wash buffer containing 1x PBS-0.05% Tween 20. Perform the washes at RT and with slow shaking. Wash the plates three times with 2 mL of buffer/well (incubate for 3 min for each wash).
2. Place 1 mL of blocking reagent (1:10) and incubate with slow agitation for 20 min.
3. Add 200 µL (1:50 dilution) of the following primary antibodies to each well: CD9 (monoclonal mouse), CD34 (polyclonal rabbit), and anti-CD63 (polyclonal goat). Incubate overnight at 4 °C.
4. Wash the plates three times again and incubate with 200 µL (1:50 dilution) of the following secondary antibodies: anti mouse IgG FITC conjugated goat, donkey anti-goat IgG DyeLight 550, and goat anti rabbit IgG Cy3.
5. Wash three times with 1x PBS-0.05% Tween 20 and counterstain the cell nuclei with 100 µL of DRAQ-7 (dilution: 17 µL in 1 mL of double distilled water) for 20 min.
6. Wash three more times and mount the slides according to steps 4.1.12-4.1.13. Store the samples protected from light and frozen until use.
7. Visualize the samples under epifluorescence confocal microscopy using the proper settings and software recommended for this equipment.

6. Expression markers of ASCs by flow cytometry

1. Adjust a single cell suspension from trypsinized or thawed cells (sub-passages 3 or 4) at a concentration of 1 x 10⁶ cells/mL of 1x PBS-5% FBS. Aliquot 100 µL with 100,000 cells in 1.5 mL centrifuge tubes.Use one aliquot without labeling for the auto-fluorescence control.
2. Add to rest all appropriate amounts of Anti-CD105 AF-594 and Anti-CD31 AF-680, according to the manufacturer's instructions. Incubate in the dark for 20 min at 4 °C.
3. Wash the excess stain with 1 mL of 1x PBS-5% FBS by centrifugation at 250 x g for 5 min and suspend in 300 µL of 1% formalin.
4. Perform sample acquisition on a flow cytometer. The gating strategy of the cells is based on FSC-A vs. SSC-A gating, single cells gated using SSC-H vs. SSC-A followed by FSC-A vs. FSC-H.
5. Use Y610-mCherry-A detector for CD105 AF-594 and R660-APC-A detector for CD31 AF-680.

7. Differentiation of ASCs to the adipogenic lineage

1. In a 6-well plate, seed 1 x 10⁴ cells (P-4) per cm² and incubate at 37 °C, 5% CO₂, until 60-80% confluence (~72-96 h). Induce differentiation, applying directly to the culture medium: 4 µM insulin, 1 µM dexamethasone 21-acetate (Dxa), and 0.5 mM of 3-isobutyl-1-methylxanthine (MIX). Change the differentiation medium every 2-3 days.
2. Prepare a stock solution of 800 µM insulin in 2 mL of sterile ultrapure water (add 20 µL of 1 N HCl to ensure complete dissolution) and store at -20 °C. Add 10 µL of insulin stock, previously diluted 1:100, and apply 10 µL at a final volume of 2 mL per well.
3. Prepare a stock solution of 1 mM Dxa in 5 mL of sterile ultrapure water (note that full dissolution does not occur). Store at 4 °C. Add 40 µL/well of a 1:4 dilution of Dxa stock.
4. Prepare a stock of 100 mM of MIX in 2.5 mL of 0.1 N NaOH, vortex, and add 40 µL of 1 N NaOH for complete dissolution. Store at -70 °C. Add 10 µL/well of MIX stock.
5. Filter the stock solutions through a 0.22 µm sterile syringe filter before storage.
6. On day 12, wash the cells three times with 1x PBS and incubate with 500 µL of 4 % formalin for 1 h at RT. Wash each well twice with distilled water followed, by 60% isopropanol for 5 min and let dry.
7. Add 0.5% oil red O diluted in 60% isopropanol (500 µL/well) and incubate for 20 min at RT. Wash with 1 mL of distilled water three times and observe under an inverted microscope.
   NOTE: For reagents, equipment, and materials required, refer to the Table of Materials.

Representative Results

Adipose tissue was obtained from adult Sprague Dawley rats aged 3-4 months old and with a body weight of 401 ± 41 g (geometric mean ± SD). A mean value of 3.8 g of epididymal and perirenal adipose tissue corresponded to the analysis of 15 experimental extractions. After 24 h of culture, cell populations remained adhered to the plastic surface and exhibited a heterogeneous morphology. The first passage was realized at 8 ± 2 days, with a yield of 1.4 ± 0.6 x 10⁶ cells in a total of eight experiments. Direct bright field observation (Figure 1) and hematoxylin-eosin staining (Figure 2) facilitated morphological characterization with light microscopy. An extensive cytoplasm was visible with elongated prolongations and abundant intracellular microfilaments, a hallmark of mesenchymal stromal cells.

ASCs expressed surface markers specifically visualized by indirect immunofluorescence in different sub-passages (1, 3, 7, and 9) (Figure 3). ASCs were 100% positive for CD9 surface markers in all sub-passages tested. The percentage is the number of positive cells with respect to the number of total cells counted in five randomly taken micrographs. The cells (100%) expressed CD63 markers in sub-passages 1, 3, and 9 (P-1, P-3, P-9), while 49.3% did in P-7. The CD34 marker was negative in passages 1, 7, and 9, but positive labeling results were observed in passage 3. In addition, immunophenotyping by FCM showed that 98.7% of the cell population was positive for CD105, while only 5.88% expressed the CD31 marker (Figure 4).

Finally, ASCs exposed to a cocktail of differentiation factors for 12 days showed their ability to differentiate toward the adipogenic lineage (Figure 5). After 48 h, we observed the first changes in the morphology; the cells reduced in size and exhibited a rounded shape. After 7 days, lipid vesicles were visible, which were positive for oil red staining 12 days after differentiation.

Figure 1: Stromal vascular fraction (SVF) extracted from rat adipose tissue and digested with 0.075% collagenase (at 24 h). (A) SVF (20x). (B) SVF followed five washes (10x). The cells adhered to the plastic surface exhibit a heterogeneous morphology: rounded, star-shaped, and fibroblastoid in appearance (inverted microscope). Scale bar represents 100 µm. Please click here to view a larger version of this figure.

Figure 2: Morphological characterization with hematoxylin-eosin staining. (A) ASCs, P-1 (10x). (B) ASCs, P-1, (C) P-3, and (D) P-9 (100x). Scale bar represents 100 µm. Please click here to view a larger version of this figure.

Figure 3: Evaluation of different expression markers for ASCs and exosomes by IF. Axis X: passages 1, 3, 7, and 9. Axis Y: CD9: anti mouse IgG FITC conjugated goat; CD63: goat anti rabbit IgG Cy3; and CD34: donkey anti-goat IgG DyeLight 550. Nuclei stained in blue with DraQ7 (40x magnification, 1x zoom). Scale bar represents 100 µm in every panel. Please click here to view a larger version of this figure.

Figure 4: ASC identification by flow cytometry. (A–C) Samples selected based on FSC-A vs. SSC-A gating, single cells gated using SSC-H vs. SSC-A followed by FSC-A vs. FSC-H. (D,E) Autofluorescence control (unlabeled cells). (F,G) ASCs labeled with anti-CD105 AF-594 (Y610 mCherry; positive marker) and anti-CD31 AF-680 (R660-APC-A detector; negative marker), respectively. Please click here to view a larger version of this figure.

Figure 5: Functional assessment of rat adipose tissue mesenchymal stromal cells. (A) Control (10x). (B) Adipogenic differentiation 10x, (C) 20x, and (D) 40x. Intracytoplasmic lipid droplets positive to oil red dye at 12 days of induction (phase contrast microscopy). Scale bar represents 100 µm. Please click here to view a larger version of this figure.

Discussion

In the last four decades since the discovery of MSCs, several groups of researchers have described procedures for obtaining MSCs from different tissues and species. One of the advantages of using rats as an animal model is their easy maintenance and rapid development, as well as the ease of obtaining MSCs from adipose tissue. Different tissue sources have been described for obtaining ASCs, such as visceral, perirenal, epididymal, and subcutaneous fat^{12,13,14,15,16}.

Regarding the extraction procedure employed here, the authors recommend that rats should weigh between 350-450 g, achievable in the first 4 months of life. When the animals weighed between 450-600 g and were up to 8 months of age, the amount of adipose tissue per rat (5.5 ± 2.1; mean ± SD) was higher; however, the number of ASCs did not increase proportionally (data not shown). These observations are in correspondence with those made by González³, who also referred populations with higher viability and adhesiveness to the culture surface obtained from the subcutaneous tissue, compared to other sources. On the other hand, ASCs from biopsy resection exhibit greater viability, frequency, and replicative capacity compared to those obtained by liposuction⁷. In the present study, the subcutaneous tissue of the rats at the ages studied was very scarce. We therefore decided to remove the adipose tissue adjacent to the epididymis and perirenal area, which are involved in the synthesis and secretion of adipokines relevant to glucose and lipid regulation, as well as inflammation¹⁶, by surgical resection.

Current protocols for isolating adipose tissue-derived MSCs rely on enzyme-free processing procedures, such as explant culture¹⁷, as well as the use of enzymatic treatments to achieve near-total tissue disaggregation¹⁸. The proposed procedure is relatively simple and includes mechanical disaggregation, enzymatic disaggregation, and successive washes to the cell suspension. The latter is performed to remove as many unrelated cells as possible from the progenitor cells, and thus obtain minimal expression (<5%) of their surface markers. Interestingly, the amounts of SVF to obtain may depend on the type of collagenase used in the enzymatic disaggregation of adipose tissue. Type I collagenase is highly recommended for adipocyte isolation, although the use of type II¹⁹ and type VIII is also reported^20,21. In the present work, we used collagenase type IV, with a low enzymatic activity, usually used to process pancreatic tissue. Thus, a lower yield of ASCs is obtained, but there is also less membrane damage. This can modify the expression of some surface markers, and thus, their functionality. On the other hand, the low split ratio used in the expansion of the culture allowed the formation of colonies and a greater proliferative capacity.

According to morphology, there are three main types of mesenchymal cells: small cells, elongated cells, and large, flattened cells with large nuclei that are slow to multiply. These forms are probably related to intrinsic qualities, such as their differentiation potential²². The morphology observed in primary cultures of ASCs are consistent with the results reported by these authors. An abundant number of microfilaments in the cytoplasm was also visible at all stages evaluated, which corroborates the fibroblastoid morphology of the ASCs obtained in the study^23,24,25. Additionally, immunophenotyping is required to confirm the mesenchymal nature of the isolated cells. The ISCT and the IFATS recommend the use of some markers, although other alternatives are also possible. It is known that MSCs can produce large amounts of exosomes²⁶ which are small vesicles secreted into the extracellular medium with a particular protein content. Due to their endosomal origin, they contain fusion and membrane transport proteins (GTPases, annexins, and flotillin), tetraspanins (CD9, CD63, CD81, and CD82), among others, also expressed on the surface of the cells from which they originate^17,18. A limitation of this study is that a broad panel of markers is not evaluated. However, the use of at least two positive and negative markers in the same test is accepted.

In this work, indirect immunofluorescence with exosomal markers revealed a positive signal from ASCs to CD9 and CD63 markers in sub-passages 1, 3, 7, and 9. Since the signal observed in passage 7 was weak, it would be important to use those markers recommended by the ISCT and the IFATS to obtain better results. CD34 is a surface antigen recognized as an endothelial and hematopoietic cell marker and a positive marker of adipose tissue SVF-derived cells. However, its expression on native ASCs correlates negatively with cell expansion in vitro²⁷. CD34+ cell percentage depends on the method of adipose tissue harvest, the degree of vascular hemorrhage, and the subsequent digestion and isolation techniques. Although ASCs consistently express different markers, their dynamics have been shown to change during in vitro expansion^28,29, as evidenced by the results obtained with the proposed methodology.

At present, there is no standardized protocol for obtaining ASCs. The results are variable, since different factors modify its morphology and functionality. The age and health status of the donor, the source, and the culture conditions of the ASCs are some of these factors. The proposed methodology is focused on the standardization of a reproducible methodology that covers the purposes of diverse investigations. The scientific community is striving to find new therapeutic options for the diagnosis, control, and treatment of various metabolic diseases, including diabetes. Therefore, the disclosure of methodological procedures is also relevant.

Materials

Amphotericin B	HyClone	SV30078.01
Analytical balance	Sartorius	AX224
Antibody anti- CD9 (C-4)	Santa Cruz	Sc-13118
Antibody anti-CD34 (C-18)	Santa Cruz	Sc-7045
Antibody anti-C63	Santa Cruz	Sc-5275
Antibody anti-Endoglin/CD105 (P3D1) Alexa Fluor 594	Santa Cruz	Sc-18838A594
Antibody anti-CD31/PECM-1 Alexa Fluor 680	Santa Cruz	Sc-18916AF680
Antibody Goat anti-rabitt IgG (H+L) Cy3	Novus	NB 120-6939
Antibody Donkey anti-goat IgG (H+L) DyLight 550	Invitrogen	SA5-10087
Antibody anti-mouse IgG FITC conjugated goat F (ab´)	RD Systems.	No. F103B
Bottle Top Filter Sterile	CORNING	10718003
Cell and Tissue Culture Flasks	BIOFIL	170718-312B
Cell Counter Bright-Line Hemacytometer with cell counting chamber slides	SIGMA Aldrich	Z359629
Cell wells: 6 well with Lid	CORNING	25810
Centrifuge conical tubes	HeTTICH	ROTANA460R
Centrifuge eppendorf tubes	Fischer Scientific	M0018242_44797
Collagen IV	Worthington	LS004186
Cryovial	SPL Life Science	43112
Culture tubes	Greiner Bio-One	191180
CytExpert 2.0	Beckman Coulter	Free version
CytoFlex LX cytometer	Beckman Coulter	FLOW-2463VID03.17
DMEM	GIBCO	31600-034
DMSO	SIGMA Aldrich	67-68-5
DraQ7 Dye	Thermo Sc.	D15106
EDTA	SIGMA Aldrich	60-00-4
Eosin yellowish	Hycel	300
Ethanol 96%	Baker	64-17-5
Falcon tubes 15 mL	Greiner Bio-One	188271
Falcon tubes 50 mL	Greiner Bio-One	227261
Fetal Bovine Serum	CORNING	35-010-CV
Gelatin	SIGMA Aldrich	128111163
Gentamicin	GIBCO	15750045
Glycerin-High Purity	Herschi Trading	56-81-5
Hematoxylin	AMRESCO	0701-25G
Heracell 240i CO2 Incubator	Thermo Sc.	50116047
Ketamin Pet (Ketamine clorhidrate)	Aranda	SV057430
L-Glutamine	GIBCO/ Thermo Sc.	25030-081
LSM software Zen 2009 V5.5		Free version
Biological Safety Cabinet Class II	NuAire	12082100801
Epifluorescent microscope	Zeiss Axiovert 100M	21.0028.001
Inverted microscope	Olympus CK40	CK40-G100
Non-essential amino acids 100X	GIBCO	11140050
Micro tubes 2 mL	Sarstedt	72695400
Micro tubes 1,5 mL	Sarstedt	72706400
Micropipettes 0.2-2 μL	Finnpipette	E97743
Micropipettes 2-20 μL	Finnpipette	F54167
Micropipettes 20-200 μL	Finnpipette	G32419
Micropipettes 100-1000 μL	Finnpipette	FJ39895
Nitrogen tank liquid	Taylor-Wharton	681-021-06
Paraformaldehyde	SIGMA Aldrich	SLBC3029V
Penicillin / Streptomycin	GIBCO/ Thermo Sc.	15140122
Petri dish Cell culture	CORNING Inc	480167
Pipet Tips	Axygen Scientific	301-03-201
Pisabental (pentobarbital sodium)	PISA Agropecuaria	Q-7833-215
Potassium chloride	J.T.Baker	7447-40-7
Potassium Phosphate Dibasic	J.T Baker	2139900
S1 Pipette Fillers	Thermo Sc	9531
Serological pipette 5 mL	PYREX	L010005
Serological pipette 10 mL	PYREX	L010010
Sodium bicarbonate	J.T Baker	144-55-8
Sodium chloride	J.T.Baker	15368426
Sodium Phosphate Dibasic Anhydrous	J.T Baker	7558-79-4
Sodium pyruvate	GIBCO BRL	11840-048
Syringe Filter Sterile	CORNING	431222
Spectrophotometer	PerkinElmer Lambda 25	L6020060
Titer plate shaker	LAB-LINE	1250
Transfer pipets	Samco/Thermo Sc	728NL
Trypan Blue stain	GIBCO	1198566
Trypsin From Porcine Pancreas	SIGMA Aldrich	102H0234
Tween 20	SIGMA Aldrich	9005-64-5
Universal Blocking Reagent 10x	BioGenex	HK085-GP
Xilapet 2% (xylazine hydrochloride)	Pet's Pharma	Q-7972-025