Primer & Oligo Design Answers After Choosing a Calculator

Use the Tm Calculator as the primary action page for vendor-style Tm checks. It lets you match salt, Mg²⁺, DMSO, and oligo concentration assumptions before you compare values from another calculator.

Example conditions: 50 mM Na⁺, 0 mM Mg²⁺, 250 nM oligo concentration. Run the Tm Calculator or review the calculation methodology.

Open Tm Calculator for the actual result

Check the method, salt assumptions, oligo concentration, and whether Mg²⁺ or DMSO corrections are enabled. Most Tm disagreements come from condition mismatch, not from the sequence itself.

What differs between tools is:

• Salt correction formula — use a method suitable for your PCR buffer
• Batch review — use batch mode when primer pairs or pools must be checked together
• Privacy — OligoPool calculations run in your browser with client-side JavaScript

For the calculation itself, open the Tm Calculator. Use this page for follow-up interpretation.

Open Tm Calculator for the actual result

Use the Primer Analyzer when you need a combined primer review that includes Tm, GC%, molecular weight, hairpins, self-dimers, hetero-dimers, and mismatch checks in one report.

For a detailed comparison, see OligoPool vs IDT — Full Feature Comparison. For immediate analysis, open the Primer Analyzer.

Open Tm Calculator for the actual result

All calculations run entirely in your browser using client-side JavaScript. Your sequences are never transmitted to any server. You can verify this using browser developer tools (Network tab). This is a key advantage over vendor tools (IDT, NEB) that process sequences on their servers. Only if you explicitly save sequences to your Library (optional account feature) is data stored, encrypted in our database.

Open Tm Calculator for the actual result

The nearest-neighbor (NN) thermodynamic method is commonly preferred for primers and probes because it accounts for stacking interactions between adjacent base pairs, not just base composition.

The Tm Calculator uses SantaLucia 1998 with Owczarzy 2008 salt correction for settings where those assumptions fit the experiment.

Calculate Tm with matched buffer settings

Differences of ±2°C between calculators are normal and come from: 1) Different parameter sets — SantaLucia 1998 vs older Breslauer 1986, 2) Different salt corrections — Owczarzy 2008 vs older SantaLucia 1998 formula, 3) Assumed oligo concentration — 0.25 µM vs 0.5 µM, 4) Initiation parameter handling — how terminal base pairs are counted.

Bottom line: If your result differs from NEB by more than 2°C, check that you're using the same salt concentrations. Na⁺ and Mg²⁺ settings cause 90% of discrepancies.

Calculate Tm with matched buffer settings

Use your actual buffer concentrations for accurate Tm prediction. Common defaults:

Critical: Changing Na⁺ from 50→100 mM shifts Tm by +3-5°C. Changing Mg²⁺ from 1.5→3 mM shifts Tm by +1.5-2.5°C. Always match your actual conditions.

Calculate Tm with matched buffer settings

For standard PCR: 55-65°C, with 58-62°C being optimal. Primer pairs should have Tm within 5°C of each other (ideally within 2°C). Set annealing temperature (Ta) 5°C below the lower Tm. For high-fidelity enzymes (Phusion, Q5): higher Tm (65-72°C) may be recommended — check the manufacturer's Ta calculator. For qPCR probes: Tm 5-10°C above the primer Tm for effective 5' nuclease assay.

Calculate Tm with matched buffer settings

Standard nearest-neighbor parameters are for unmodified DNA. Terminal modifications (5'-phosphate, biotin, fluorescent labels at 5' end) have negligible effect on Tm (<0.5°C). However, backbone modifications significantly affect stability: LNA (+2-6°C per substitution), phosphorothioate (-0.5°C per substitution), 2'-O-methyl RNA (+1-2°C per substitution). The calculator supports unmodified DNA/RNA. For modified oligos, use the calculated Tm as a baseline and adjust empirically.

Calculate Tm with matched buffer settings

Use these ΔG values as practical review points, then weigh the structure location and assay conditions:

Check your sequences with the Secondary Structure Predictor. For a detailed tutorial, see How to Detect and Fix Secondary Structures.

Run Secondary Structure Predictor

Strategies ordered by effectiveness:

1. Shift the primer binding site by 2-5 bases upstream or downstream — often eliminates the hairpin without changing target specificity
2. Introduce silent mutations (for gene assembly oligos) — change G→A or C→T at non-critical positions to break the complementary stem
3. Shorten the primer — remove bases involved in the self-complementary region (maintain Tm >55°C)
4. Add DMSO (3-10%) to the reaction — destabilizes secondary structures by 0.5-0.7°C per 1% DMSO
5. Raise annealing temperature — above the structure's Tm, favoring target binding over self-folding

For 3' end dimers specifically: avoid 3' ends with >3 consecutive G/C bases. This is the single most impactful rule for preventing primer-dimer artifacts.

Run Secondary Structure Predictor

A hairpin is when a single strand folds back on itself, forming a stem-loop structure (intramolecular). A self-dimer is when two copies of the same sequence bind to each other (intermolecular). A cross-dimer (hetero-dimer) is when two different sequences (e.g., forward and reverse primers) bind to each other. All three compete with the intended target binding, reducing PCR efficiency. 3' end involvement is most critical — dimers at the 3' end are extended by polymerase, creating primer-dimer artifacts visible as ~40-100 bp bands on gels.

Run Secondary Structure Predictor

Not always. Structures with ΔG > -2 kcal/mol are generally harmless. Structures in the 5' overhang region (outside the target-binding portion) are usually acceptable. Temperature context matters: a structure stable at 25°C but unstable at your annealing temperature (55-65°C) will not interfere with PCR. For hybridization probes (FISH, ISH), structures are less critical because longer hybridization times overcome kinetic barriers. Focus on 3' end structures — these are always problematic because they directly block polymerase extension.

Run Secondary Structure Predictor

Follow this systematic 5-step checklist:

For detailed guidance with examples, see the primer validation checklist.

Open Primer Analyzer for full primer review

For PCR primers: 40-60% is ideal, with 45-55% being optimal. For qPCR probes: 50-60% provides good stability. For oligo pools/libraries: keep GC uniform across all sequences to avoid representation bias. Avoid extremes: <30% GC produces unstable duplexes with low Tm; >70% GC promotes secondary structures (G-quadruplexes, hairpins) that reduce synthesis yield and binding efficiency. Use the GC Content Analyzer to check your sequences before ordering.

Open Primer Analyzer for full primer review

It depends on your application:

• Single primer Tm: Tm Calculator — nearest-neighbor with salt correction
• Primer pair analysis: Primer Analyzer — Tm, dimers, and specificity in one tool
• Hairpin/dimer check: Secondary Structure Predictor — ΔG calculations with visual output
• Library/pool QC: Batch Sequence QC — validate 10,000 sequences at once
• Resuspension/dilution: Dilution Calculator — concentration calculations
• Everything at once: Oligo Properties Calculator — Tm, GC%, MW, ε₂₆₀ in one view

Open Primer Analyzer for full primer review

Formula: Volume (µL) = nmoles / (target µM) × 1000. Example: 100 nmol oligo to 100 µM stock = 100/100 × 1000 = 1000 µL (1 mL) in TE buffer (10 mM Tris, 0.1 mM EDTA, pH 8.0). For accurate quantification after resuspension, measure A₂₆₀ absorbance — 1 OD₂₆₀ ≈ 33 µg/mL for single-stranded DNA. Use the Molecular Weight Calculator to get the extinction coefficient (ε₂₆₀) for precise concentration determination via Beer-Lambert law: Concentration = A₂₆₀ / (ε₂₆₀ × path length).

Open Primer Analyzer for full primer review

An oligo pool is a complex mixture of thousands to millions of unique oligonucleotides synthesized in a single reaction using array-based synthesis. Use pools when you need >100 unique sequences for the same experiment (CRISPR libraries, NGS panels, mutagenesis, gene assembly). For <100 sequences or when you need each oligo individually (PCR primers, probes), order individual oligos instead.

Start with the Oligo Pool Guide for the full design, QC, vendor, and ordering path. Use Oligo Pool vs Individual Oligos when the first decision is whether pooled synthesis is appropriate.

Open the Oligo Pool Guide

Use the Oligo Pool Vendor Comparison for vendor selection and the vendor specification notes for documented product-page details.

Open the Oligo Pool Guide

Run these checks before ordering to avoid costly redesign:

1. Upload all sequences to Batch Sequence QC — checks GC%, Tm, homopolymers, length
2. Target >90% pass rate (for CRISPR screens, aim >95%)
3. Check Tm uniformity — pool Tm CV should be <3°C for functional assays
4. Run secondary structure check on flagged sequences
5. Use Vendor Format Adapter to generate the correct order file format

Open the Oligo Pool Guide

Run Batch Sequence QC before export

We support FASTA (single-line and multi-line), CSV, TSV, and plain text (one sequence per line). The Format Converter tool auto-detects input format and converts between them. For vendor ordering: use the Vendor Format Adapter to generate IDT, Twist, GenScript, or Dynegene-specific order files.

Run Batch Sequence QC before export

Yes. Most tools support CSV/Excel export. Batch QC generates comprehensive reports with per-sequence details and pool-level statistics. The Vendor Format Adapter exports ready-to-upload order files for each supported vendor.

Run Batch Sequence QC before export

Run Batch Sequence QC before export