Agilent yeast DNA arrays (4x44k platform)
Maitreya Dunham August
2007
hybrid of Brown and deRisi
lab protocols and various Agilent 60-mer oligo microarray processing (SSPE
wash) protocols
Remember that the arrays
come 4 on a slide.
This labeling protocol
seems to be rather sensitive to DNA quality. I use the Winston and Hoffman prep with good results. If you're worried about quality, use
the Zymo genomic DNA kit, or a Qiagen kit. The Zymo kit can also be used to make DNA from colonies.
Measure starting DNA
concentration with a fluorometer.
Once it's been purified with the Zymo columns, the spectrophotometer
seems to be reasonably accurate.
Bring 4 µg DNA to 100µl in
a 1.5mL eppendorf tube.
Sonicate 30 pulses power
level 1, 1 second on/1 second off.
Run 2 µl on a gel to check
fragmentation. Fragments should be
a smear around 1 kb.
Purify with zymo DNA clean
and concentrator 5 kit.
Elute in 20 µl water.
Nanodrop 1 µl.
DNA can be stored -20C.
Bring 2 µg to 21µl with
water.
Add 20 µl 2.5X random
primer/reaction buffer mix:
|
STOCKS: |
1X: |
125mM Tris pH 6.8 |
0.5M Tris, pH 6.8 |
5 µl |
12.5mM MgCl2 |
50mM MgCl2 |
5 µl |
25mM 2-mercaptoethanol |
0.143M 2-mercaptoethanol
(dilute fresh) |
3.5 µl |
750µg/mL random nonamers |
5µg/µl random nonamers |
3 µl |
|
Water to 20 µl |
3.5 µl |
95C 5 minutes.
Ice 5 minutes.
Add 5µl 10X dNTP mix (in
TE, pH 8.0):
For dCTP Cy dyes: 1.2mM each dATP, dGTP, dTTP, and 0.6mM
dCTP
For dUTP Cy dyes: 1.2mM each dATP, dGTP, dCTP, and 0.6mM
dTTP
Add 3µl appropriate
Cy-dNTP.
Add 1µl Klenow (5U/µl).
Incubate 37C for 2 hours.
Add 5µl 0.5M EDTA pH 8.0.
Ice.
Purify using zymo columns
with 0.5 ml binding buffer.
Elute in 25 µl water.
Nanodrop 1 µl to check
yield and dye incorporation.
Dye incorporation should
be ~20 pmol/µg.
You may want to randomize
the arrays that are neighbors on the arrays. A simple way to do this in Excel is to list the samples in
one column and the function =RAND() into each cell in the neighboring column. Copy the random number column, then,
with the column still selected, paste special -> values so that the cells
won't recalculate. Then, sort both
columns by the random number. List
the arrays in a third column next to the sorted list. A01 is near the barcode and A04 is farthest from the
barcode.
Final hybe reaction will
be
Cy3-labeled DNA |
100ng |
Cy5-labeled DNA |
100ng |
Water |
to 44µl |
10X Agilent Blocking Agent |
11µl |
2X Hi-RPM hybridization buffer |
55µl |
TOTAL VOLUME |
110µl |
VOLUME LOADED |
100µl |
Add 100ng Cy3-labeled DNA
and 100ng Cy5-labeled DNA
Add water to bring the
total volume to 44µl
Add 11µl Agilent 10X
Blocking Agent (prepare 10X Blocking Agent according to instructions that came
with the tube).
95C for 5 minutes (process only 4 samples at a time)
Cool @ room temperature
for 5 minutes
Add 55µl 2X Hi-RPM
hybridization buffer, mix by pipetting
Spin down
Load 100µl onto the gasket
slide:
Place a backing slide,
Agilent side up, in a hybe chamber.
Pipet the whole volume of
probe, avoiding bubbles, onto the center of one gasket area. Don't eject the last µl or two in order
to avoid bubbles. Spread it around
as you pipet, but not too close to the gasket.
Do the same for the other
gasket area with the next probe.
Remove the array from the
box. The Agilent side is the Array
side, and so should face down, onto the probe. Carefully lower the array over the gasket slide, keeping it
flat.
Once the array is resting
on the gasket slide, place the top of the hybe chamber, and slide the screw
over the assembly. Tighten the
screw all the way down, finger tight.
Look through the back of
the chamber and rotate the slide.
There should be one big bubble that moves freely. There may be one big bubble and a
couple of little ones stuck to the sides.
If they are small and isolated, don't worry too much about them. You will probably do more harm than
good trying to remove them. If
they seem like they'll interfere with the array, you can try knocking the array
with the heel of your hand to dislodge them.
Put the array in the hybe
oven. Make sure to balance the
rotisserie.
Hybe 17 hrs. @ 65C, 20RPM
Prepare your wash
solutions. Be aware of array
materials that may be for RNA only use.
Wash A (1 L)
add in this order:
700 ml |
Water |
300 ml |
20X SSPE |
0.25 ml |
20% N-lauroylsarcosine |
Filter. Shake to mix.
Wash B (1 L)
add in this order:
997 ml |
Water |
3 ml |
20X SSPE |
0.25 ml |
20% N-lauroylsarcosine |
Filter. Shake to mix.
Rinse the wash chambers,
racks, and stirbars with water.
Set up:
two Wash A chambers, one
with a rack and a stirbar on a stirplate.
one Wash B chamber with a
stirbar on a stirplate.
one acetonitrile chamber
with a stirbar on a stirplate.
For all stirring steps,
the wash liquid should be visibly turbulent. Make sure the entire slide is submerged at all times.
Disassemble each hybe
chamber one at a time. Use the
plastic tweezers to gently wedge open the sandwich while submerged in Wash
A. Transfer slide to the rack in
the other Wash A chamber. Leave a
gap between each slide and between the slides and the wall.
Once all the slides are in
the rack, stir for 1 min.
Start stirring Wash B.
Transfer the rack into
Wash B and stir for exactly 1 min.
Don't worry about transferring some Wash A into Wash B.
Start stirring the
acetonitrile.
Quickly transfer the rack into
the acetonitrile, draining off some of the Wash B as you go.
Let stir 30 sec. Slowly and evenly pull the rack out of
the acetonitrile. If you see
droplets remaining on the slides, submerge them and try again.
Set the rack on a kimwipe.
Load the slides into
scanning holders, Agilent side up and barcode sticking out, blotting excess
acetonitrile if necessary. The
scanner scans through the back of the slide. Don't touch anywhere but the edges and the barcode.
Scan no more than 5 slides
at a time to avoid ozone in the scanner.
You can reuse the wash
buffers for more slides, replacing the first Wash A for every batch.
Open the Agilent scan
control program. If the lasers
refuse to warm up, power cycle the scanner.
Place the slides in the
scanner, noting the slot numbers.
Select the appropriate
slot numbers from the pulldown menus on the upper left.
Select the directory
column and click edit values.
Browse to find the directory you want to save in. Hit set. The column values should change.
Check the default
preferences for the correct scanning area (61 x 21.6 mm), resolution (5 µm), laser power (100% each) and with the split and
rotate box not checked.
Scan.
Open the scanned tif with
the Agilent feature extraction software.
Run the appropriate
protocol.
Check the visual results
to make sure it looks ok. I
usually check that it's aligned properly, and that the flagged spots make some
sense. If you get a larger than usual
number of outlier spots, make a note of it.