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31 protocols using oil red o

1

Oil Red O Staining of Lipid Droplets

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The cells were washed with DPBS 3 times and fixed in 4% paraformaldehyde solution for 15 min. Oil red O (Sigma, St. Louis, MO, USA) staining solution (60% stock solution and 40% deionized water), incubated at room temperature for 10 min before use. The cells were briefly washed with deionized water and rinsed once with 60% isopropanol. Oil red O staining solution was added to the plate and incubated for 10 min. The cells were rinsed with 60% isopropanol to redissolve the Oil red O. A microscope (TH4-200, Olympus, Tokyo, Japan) was used to observe Oil red O-stained cells.
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2

Hepatic Steatosis Histological Assessment

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A small portion of frozen liver tissue (n = 10) was cut and embedded with precooled optimal cutting compound (Torrance, CA, USA) for cryostat sectioning at 6 μm. The sections were mounted on microscope slides then fixed with 10% formaldehyde solution. The samples were then stained with Haematoxylin and Eosin (H&E) or Oil Red O (Sigma-Aldrich, St. Louis, MO, USA). H&E-stained slides were observed under light microscopy (Olympus, BX51 microscope, Tokyo, Japan) to investigate the architecture of liver and hepatocyte steatosis. Images were captured using an Olympus digital camera (DP70, Tokyo, Japan) with a sample size at least 80 fields per group (original magnification, ×400, 36-bit colour, 1280 × 1024 pixels). Liver steatosis was graded with semiquantitative estimation of the percentage of lipid-laden hepatocytes, according to the method previously described [18 (link)]. At least 5 different high-power fields (original magnification, ×400) were graded in a blinded way. Stained Oil Red O slides were visualized with the Olympus microscope and images were captured with digital camera (DP70, Tokyo, Japan) using Image-Pro 6.2 software (Media Cybernetics, Inc., MD, USA).
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3

Visualizing Lipid Droplets in Atrial Myocytes

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To visualize lipid droplets, the HL-1 atrial myocytes were stained with Oil Red O (ScyTek Laboratories, Logan, UT, USA) according to the manufacturer’s directions. Sections were mounted and visualized with a Dmi3000 microscope. The Oil Red O-stained area per myocyte was analyzed by Cellsens Dimension (Olympus, Tokyo, Japan), with at least 60 randomly-chosen myocytes for each experiment. Stretched and non-stretched myocytes were compared in five experiments.
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4

Adipogenic Differentiation of Cells

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Freshly sorted cells were expanded as described above. After 5–7 days, medium was changed to adipogenic induction medium consisting of DMEM + 10% FBS + 1% penicillin/streptomycin + 1mM Dexamethasone (Sigma) + 100nM Insulin (Sigma) + 1mM Roziglitazone (Cayman Chemical) + 0.5 mM 3-isobutyl-1-methylxanthine (Sigma) for 2 days, and then replaced with adipogenic differentiation medium consisting of DMEM + 10% FBS + 1% penicillin/streptomycin + 100nM Insulin. Cells were kept in differentiation medium for 6 days, and then fixed with 4% Paraformaldehyde and stained with Oil Red O (Sigma) for one hour at room temperature [11 (link)]. Oil Red O staining of lipid droplets within adipocytes was analyzed by standard microscopy using an Olympus IX51 inverted microscope.
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5

Quantification of Adipocyte Lipid Content

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3T3-L1 cells were cultured in 60 mm diameter dishes (8.4×104 cells/dish) and treated with NNMT inhibitor dissolved in culture media with/without adipogenic factors (1 mM IBMX, 1 µM dexamethasone, 10 µg/ml of insulin) during each of the scheduled media changes during the differentiation process (described above). On day 9 post-differentiation, cells were subjected to quantitative oil red O (Thermo Fisher Scientific; Waltham, MA, USA) staining as adapted and modified from published protocols.[12 (link)] Briefly, cells were washed twice with PBS, fixed with 10% formalin for 30 min at room temperature, and stained with oil red O working solution (~0.2% oil red O in 99% isopropanol) for 30 min. Cells were then washed five times or with sterile water until unincorporated oil red O stain was completely removed. Images of oil red O staining in control and inhibitor-treated cells were digitally photographed using a light microscope (Olympus BX41; Tokyo, Japan). After image capture, 2-propanol (3.5 mL) was added to each dish for 10 min to dissolve the oil red O stain and absorbance was quantified in a plate reader set at 492 nm wavelength. To ensure the absorbance from oil red O staining was within the linear detection range of the plate reader, a calibration curve was established for oil red O staining in adipocytes using a previously described protocol.[23 (link)]
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6

Quantifying Myocardial Lipid Accumulation

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Left atrial tissues were sliced into 8-µm sections, stained with Oil red O to visualize lipid accumulation (ScyTek Laboratories, Utah, USA) according to the manufacturer’s directions. Sections were mounted and visualized using an Olympus BX51 microscope. The Oil red O stained area per myocyte was analyzed by Cellsens Dimension (Olympus, JAPAN) with at least 100 randomly chosen myocytes per each sample.
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7

Adipogenic Differentiation of hMSCs

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The cells from passage three were cultured in adipogenic induction medium (hMSC Differentiation BulletKit; Lonza, Walkersville, MD, USA) at 37°C in 5% CO2/95% air and were maintained for three weeks, and the culture medium was replaced three times every seven days. Intracellular lipid droplets indicating adipogenic differentiation were confirmed by Oil Red O (Sigma-Aldrich, São Paulo, Brazil) staining with 0.5% Oil Red O in methanol and observation under an optical microscope (CK40, Olympus, São Paulo, Brazil).
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8

Oil Red O Staining for Lipid Quantification

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The culture medium was removed and the cells were fixed with 4% paraformaldehyde (Solarbio, Beijing, China) for 30 min. After adding oil red O (Sigma) which was soluble in isopropanol for 10 min and rinsing with PBS, the oil red O staining results were observed and photographed under the microscope (Olympus, IX71, Tokyo, Japan). Dyeing areas were counted with the Image J software (National Institutes of Health, Bethesda, MD), and 3 images were used for analysis each time [13 (link)].
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9

Cryosectioning and Oil Red O Staining Protocol

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Tissue samples of brain, lung, heart and kidney size 1 × 1 × 0.3 cm were frozen in the OCT compound on dry ice. Sections 8 µm thick were cut at − 20 °C by use of a cryostat (Cryostar NX50, Thermo Scientific, USA). Three to five serial sections were mounted on poly-L-lysine coated slides and air-dried before staining. The sections were fixed with 4% neutral buffered formalin for 20 min., rinsed in tap water, following by few dips in 60% isopropanol and incubation in 0.5% Oil Red O working solution (30 mL 0.5% Oil Red O (Sigma-Aldrich, St Louis, MO) stock solution diluted with 20 mL 1% dextrin aqueous solution) for 20 min. After incubation samples were shortly rinsed in 60% isopropanol and counterstained with Gill III modified Hematoxylin solution (Merck KGaA, Darmstadt, Germany) for 15 s, rinsed 3 × 30 s with distilled water, blued, and mounted with glycerin jelly. Oil Red O stained images were captured by using Olympus SC180 digital camera (Olympus Europa GmbH, Hamburg, Germany) installed on Olympus BX51 light microscope.
The images were processed by using Olympus cellSens Entry software Soft Imaging System GmbH, Munster, Germany). The staining methods are described in Bancroft’s Theory and Practice of Histological Techniques [23 ].
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10

Alisol B Modulates Lipid Metabolism in Mouse Hepatocytes

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Mouse primary hepatocytes were exposed to 0.2 mM palmitate (PA) with or without Alisol B for 48 h. After being fixed in 4% paraformaldehyde for 30 min, cells were stained with Oil Red O (Cat#71029781, Sinopharm Chemical Reagent Co., Shanghai, China) working solution for 20 min and subsequently stained with hematoxylin solution for 3 min. The respective images of Oil Red O staining were captured with an Olympus IX73 microscope at 200× magnification. To evaluate hepatic fatty acid uptake, mouse primary hepatocytes were treated with or without Alisol B for 48 h and then incubated with 100 nM BODIPY-C16 (Cat#3821, Thermo Fisher Scientific, Waltham, MA, USA) for 5 min. After being fixed with 4% paraformaldehyde for 30 min, the hepatocytes were incubated with DAPI to stain nuclei for 3 min, and the images of BODIPY-C16 fluorescence were captured at 600× magnification with an Olympus FV1000-SIM microscope.
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