1. Single cell preparation: Isolate single cells, deposit into 0.2-ml PCR tubes containing 2.5 µl PBS, place tubes on dry ice, store at -80°C. 2. Whole genome amplification: In PCR workstation, add 1 µl exo-resistant random primers and 3 µl lysis buffer (400 mM KOH, 100 mM DTT, 10 mM EDTA) to PCR tube with single cell. Flick mixture, spin down, keep on ice for 10 min. Add 3 µl stop buffer (400 mM HCl, 600 mM Tris-HCl pH 7.5) to neutralize lysis buffer, keep on ice for 2 min. Add 32 µl master mix (30 µl MDA reaction buffer, 2 µl Phi29 polymerase), mix gently. Incubate at 30°C for 1.5 hr, 65°C for 3 min. 3. Amplified product purification: Purify product with 75.6 µl AMPureXP-beads, mix by pipetting, leave at room temperature for 5 min, use magnetic separator until clear. Remove clear liquid, wash beads twice with fresh 80% ethanol. Air-dry beads for about 5 min, avoid cracking. Elute beads with 32 µl nuclease-free water, use magnetic separator until clear, transfer 30 µl clear liquid to clean tube. Store purified product at 4°C (short-term) or -20°C (long-term). 4. Concentration and size measurement: Dilute purified product 10-20 times, quantify with Qubit (yield 10-12 µg). Check product size by agarose gel electrophoresis (1.0% agarose gel, 1.0% TBE, 100V, 40 min). A bright band over 10 kb is desirable. 5. Estimation of amplification uniformity: Dilute purified product and unamplified genomic DNA to 1 ng/µl. Prepare 96-well plate with PCR mixture: 5 µl Fast Sybr green master mix, 1 µl locus-specific primers, 2 µl nuclease-free water, 2 µl diluted DNA. Seal plate, spin down, incubate: 95°C for 20s, 40 cycles of 95°C for 3s, 60°C for 30s. Calculate relative uniformity values (RUVs) for 8 loci, select samples with RUV values for at least 6 of 8 loci between 0.25-4 for library construction.