qPCR Efficiency Determination Protocol

Optimization of qPCR Conditions

Optimization of qPCR conditions is important for the development of a robust assay. Indications of poor optimization are a lack of reproducibility between replicates as well as inefficient and insensitive assays. The two main approaches are optimization of primer concentration and/or annealing temperatures.

Once an assay has been optimized, it is important to verify the reaction efficiency. This information is important when reporting and comparing assays. In this example protocol, the assay efficiency is compared over a wide and narrow dynamic range of cDNA concentrations. In practice, it is common to select a single range to test depending on the expected range of target in the samples, so the protocol given can be adjusted according to the requirements of the experiment. In this example the efficiency is calculated using both 10-fold and 2-fold dilution series. The standard curve should encompass the expected range of expression for the genes of interest Note that the proportionality of the cDNA yield with respect to RNA input is linear when using the ReadyScript^® RT kit, so this experiment can be adapted to RT-qPCR if using that system by 1) diluting the RNA and running the RT reactions and 2) then running qPCR on each of the resulting cDNA samples (see Reverse Transcription for examples). However, this is not always the case and does not apply for all Reverse Transcription kits or protocols. This should be verified before adapting this protocol to an alternative kit

Equipment

• Quantitative PCR instrument
• Laminar flow hood for PCR set up (optional)

Reagents

• DNA to be used as the standard curve template (e.g., cDNA, gDNA or a synthetic template).
• KiCqStart SYBR^® Green ReadyMix™ (KCQS00/KCQS01/KCQS02/KCQS03—depends on instrument,
  Table P4-6).
• PCR grade water: PCR grade water (W1754 or W4502) as 20 mL aliquots; freeze; use a fresh aliquot for each reaction.
• Forward and reverse primers for test genes (stock at 10 μM).

Supplies

• Sterile filter pipette tips
• Sterile 1.5 mL screw-top microcentrifuge tubes (CLS430909)
• PCR tubes and plates, select one to match desired format:
  • Individual thin-walled 200 μL PCR tubes (Z374873 or P3114)
  • Plates
  - 96-well plates (Z374903)
  - 384-well plates (Z374911)
  • Plate seals
  - ThermalSeal RTS™ Sealing Films (Z734438)
  - ThermalSeal RT2RR™ Film (Z722553)

Notes for this Protocol

• cDNA is generated using random priming or oligo-dT method (see Standard Reverse Transcription Protocol (Two-step)). The RT product is diluted to prepare the standard curves (1:2 and 1:10 are given as examples). RNA can also be diluted and cDNA synthesized from each dilution using the ReadyScript^® kit or a one-step RT-qPCR approach can be adopted by diluting RNA and following the one-step RT-qPCR approach in Reverse Transcription Protocol (One-step SYBR^® Green I Dye Detection) and Reverse Transcription Protocol (One-step Probe Detection). Alternatively, DNA templates can be substituted such that the expected C_q range is within C_q 15 to C_q 38.
• Each concentration of the serial dilutions will be run as duplicate reactions.

Method

1. Prepare a qPCR master mix that is sufficient for 40 reactions following Table P16-40. This allows for extra to
accommodate pipetting errors since 32 reactions will be run (Table P16-41).

2. Dilute the DNA through a series of 1:10 and 1:2 covering 7 dilution points for each series (Table P16-41, Plate Layout for DNA Dilution).

3. Add 5 μL of appropriate template dilution to the defined wells (Table P16-41, Plate Layout for DNA Dilution).

4. Add 15 μL of master mix to each well (Table P16-41).

5. Cap tubes or seal the plate and label. (Make sure the labeling does not obscure instrument excitation/detection
light path).

6. Run samples according to the two-step protocol below. Steps 1–2 are repeated through 40 cycles. Follow
amplification with a standard dissociation curve analysis.

Note: Use standard dissociation curve protocol (data collection).