Localization of particular sequences within genomic DNA is usually accomplished by the transfer techniques described by Southern (1975). Genomic DNA is digested with one or more restriction enzymes, and the resulting fragments are separated according to size by electrophoresis through an agarose gel. The DNA is then denatured in situ and transferred from the gel to a solid support (usually nitrocellulose filter or nylon membrane). The relative positions of the DNA fragments are preserved during their transfer to the filter. The DNA attached to the filter is hybridized to radiolabeled DNA or RNA, and autoradiography is used to locate the positions of bands complementary to the probe. A sequence of 1000 bp that occurs only once in the mammalian genome can be detected in an overnight exposure if 10 µg of genomic DNA is transferred to the filter and hybridized to a probe several hundred nucleotides in length.

Ⅰ. Restriction digestion of genomic DNA (overnight )

Complete digestion of genomic DNA is crucial but difficult. The average restriction fragment size varies according to the length of the recognition sequence, and also the GC content of the recognition site; AT rich sites occur more frequently. You don't want to see DNA hanging up at the mobility limit of the gel; you do want to see a few tight bands within the smear (these are repetitive sequences). To ensure complete digests, dilute the digest into a larger volume (thus diluting the enzyme inhibitors) and then precipitate and resuspend the cut DNA in the desired volume. You can try using 10 units of restriction enzyme per µg of DNA and digesting overnight (note: this is only useful for stable restriction enzymes- the Biolabs catalog has a table showing the stability of various enzymes). EcoRI is excellent at cutting genomic DNA, HindIII is good, others vary. After digestion, run an aliquot on an analytical gel to check the digestion: should see a smear with a bell-shaped distribution of intensity. EcoRV and XbaI are other 6-cutters with AT-rich recognition sites that work okay.

1.Cut off and autoclave pipette tips for handling high-molecular-weight genomic DNA.

2.Digest 10 µg genomic DNA in 400 µl total volume with 3 units restriction enzyme per µg DNA at 37℃ for overnight.

(For random primer labeling you will also need to cut out the cDNA probe from vector.)

(To ensure homogeneous dispersion of the genomic DNA: (a) allow the DNA to stand at 4℃ for several hours after dilution and addition of 10 x restriction enzyme buffer, (b) gently stir the DNA solution from time to time, (c) after adding restriction enzyme, gently stir the solution for 2-3 minutes at 4℃ before warming up to 37℃, (d) after digestion for 30 minutes, add a second aliquot of restriction enzyme and stir as described above)

3.Add 0.1 volume (10µl) 3 M sodium acetate, mix well. Add 2.5 volumes ice-cold 100% ethanol. Precipitate at -80℃ for 1 hour . Spin in microfuge at high speed for 20 minutes. Discard supernatant, air-dry for 5 minutes. Resuspend in 15 µl 10mM Tris pH 7.5.

(Residual ethanol can cause the DNA sample to 'crawl' out of the well when loaded onto the gel. Heating the solution of redissolved DNA to 65-70℃ in an open tube for 10 minutes can usually drive off most of the ethanol.)

4.Add 3 µl 6 x DNA-loading buffer (total volume 18 µl).

Ⅱ. Agarose gel electrophoresis (6-16 hours)

1.Pour a 0.8% agarose gel.

(Mix 1.6 grams ultra pure agarose in 200 ml 1X TAE (0.8%). Add 2 µl 1% ethidium bromide solution . Pour into long (20 cm) gel rig)

2.Prepare DNA size markers.

(2µl lambda HindIII (1µg) + 1µl 100 bp ladder (1µg) , 9µl H2O, 3µl 6x DNA loading buffer)

3.Optional: Prepare positive control.

(Mix 10µg digested genomic DNA with 1-10 pg plasmid containing the cDNA for which will be probed. Load into lane far outside from samples to avoid contamination or interference with sample hybridization)

4.Submerge gel in 2000 ml 1X TAE with 0.5 µg/ml ethidium bromide.

(i.e. 40 ml of 50 x TAE, 100 µl of 1% ethidium bromide stock solution, dH2 O ad 2 liter)