DAPI Counterstaining Protocols
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实验试剂
Choose one of the following forms of DAPI:
DAPI dihydrochloride (MW = 350.3)
DAPI dihydrochloride, FluoroPure™ grade (=98% pure)
Phosphate-buffered Saline (PBS)
Optional: antifade reagent (ex. ProLong® Gold or SlowFade® Gold reagent)
Staining buffer (100 mM Tris, pH 7.4, 150 mM NaCl, 1 mM CaCl2 , 0.5 mM MgCl2 , 0.1% Nonidet P-40). A 1 mL volume will be required for each cell sample.
Optional: antifade reagent (ex. ProLong® Gold or SlowFade® Gold reagent)
实验步骤
1. Adherent Cells for Fluorescence Microscopy
Use the fixation protocol appropriate for your sample. DAPI staining is normally performed after all other staining. Note that fixation and permeabilization of the sample are not necessary for counterstaining with DAPI.
i. Equilibrate the sample briefly with phosphate-buffered saline (PBS).
ii. Dilute the DAPI stock solution to 300 nM in PBS. Add approximately 300 µL of this dilute DAPI staining solution to the coverslip preparation, making certain that the cells are completely covered.
iii. Incubate for 1–5 minutes.
iv. Rinse the sample several times in PBS. Drain excess buffer from the coverslip and mount. We recommend using a mounting medium with an antifade reagent such as our SlowFade® Gold antifade reagent or ProLong® Gold antifade reagent.
v. View the sample using a fluorescence microscope with appropriate filters.
2. Cells in Suspension for Flow Cytometry
Use the fixation protocol appropriate for your sample, or use the following protocol:
i. Collect a cell suspension of 2 × 105 to 1 × 106 cells.
ii. Pellet the cells by centrifugation and discard the supernatant.
iii. Tap the tube to resuspend the pellet in the residual liquid and add 1 mL of PBS at room temperature.
iv. Transfer the full volume of resuspended cells to 4 mL of absolute ethanol at –20°C by pipetting the cell suspension slowly into the ethanol while vortexing at top speed. Leave the cells in ethanol at –20°C for 5–15 minutes.
v. Pellet the cells by centrifugation and discard the ethanol.
vi. Tap the tube to loosen the pellet and add 5 mL of PBS at room temperature. Allow the cells to rehydrate for 15 minutes.
i. Dilute the DAPI stock solution to 3 µM in staining buffer (100 mM Tris, pH 7.4, 150 mM NaCl, 1 mM CaCl2 , 0.5 mM MgCl2 , 0.1% Nonidet P-40). A 1 mL volume will be required for each cell sample.
ii. Centrifuge the cell suspension (from step 2.6) and discard the supernatant. Tap to loosen the pellet and add 1 mL of DAPI diluted in staining buffer.
iii. Incubate for 15 minutes at room temperature.
iv. Analyze by flow cytometry in the presence of the dye. If the cells are to be viewed by fluorescence microscopy, centrifuge the sample, remove the supernatant and resuspend cells in fresh buffer. Apply a drop of the suspension to a microscope slide, cover with a coverslip and view.
Prepare the specimen according to standard procedures.5,6 Briefly rinse the final preparations in dH2O before counterstaining to remove residual buffer salts from the slide. This final rinse will help reduce nonspecific background staining on the glass. Allow the preparation to air dry.
i. Dilute the DAPI stock solution to 30 nM in PBS. Pipet 300 µL of this staining solution directly onto the specimen. A plastic coverslip can be used to distribute the dye evenly on the slide.
ii. Incubate the specimen in the dark for 30 minutes at room temperature.
iii. Carefully remove the coverslip and rinse the specimen briefly with PBS or dH2 O to remove unbound dye.
iv. Remove excess liquid from the slide by gently blotting around the sample with an absorbent tissue.
v. Place a glass coverslip on the slide and seal the edges with wax or nail polish. Alternatively, the preparation can be mounted in an antifade reagent according to the manufacturer’s directions.
vi. View the sample using a fluorescence microscope with appropriate filters.
