🧬 PGT Laboratory Turnaround Time Workflow Simulator

Biopsy Sample Preparation & Shipment

The turnaround clock starts the moment a trophectoderm biopsy tube is capped in the IVF lab. Every embryo represented by that tube is already vitrified and waiting in liquid nitrogen storage — so from this point forward, every day the sample spends in transit or in a queue is a day added before a transfer can be scheduled.

• 5–10: Cells per TE biopsy (trophectoderm cells)
• −78°C: Shipment temperature (dry ice sublimation)
• 24–48h: Typical courier transit (clinic → reference lab)
• 4–6: Chain-of-custody checkpoints (scan events per sample)

Why the embryo is already frozen before results exist

Trophectoderm biopsy is performed on Day 5, 6, or 7 blastocysts, removing 5–10 cells from the outer layer that will become placenta — the inner cell mass that forms the fetus is left untouched. Because a genetic result cannot be generated fast enough in most labs to keep pace with the narrow blastocyst transfer window, the embryo is vitrified (ultra-rapid cryopreservation) immediately after biopsy and stored in liquid nitrogen while the tube of cells is sent for testing.

This "biopsy-then-freeze-then-test" workflow, sometimes called a freeze-all strategy, decouples the embryology timeline from the genetics timeline. It also means the turnaround time of the genetics lab has zero effect on embryo viability — the embryo is stable in storage for years if needed — but it has a very direct effect on how soon the patient can start a frozen embryo transfer (FET) cycle.

Because embryos are already safely vitrified, laboratories are not racing against embryo viability — they are racing against patient time, cycle scheduling, and clinic throughput. A 5-day versus 10-day result changes when the FET can be booked, not whether the embryo survives.

Packaging, cold chain, and chain-of-custody

Each biopsy tube contains the cells suspended in a small volume of buffer or PBS, sealed in a cryotube, and labeled with a unique patient/embryo identifier that must match records at every downstream step. Tubes are placed in a rigid shipping container with sufficient dry ice to maintain a frozen or refrigerated state for the entire transit window, cushioned against physical shock.

Chain-of-custody documentation accompanies the shipment: who packed it, when it left the clinic, tracking number, temperature logger data, and a signed receipt confirming condition on arrival at the reference lab. Reference labs typically log 4–6 discrete checkpoints — pack, courier pickup, in-transit scan, facility receipt, accessioning, and freezer log-in — so that any delay or temperature excursion can be traced to a specific link in the chain.

Some large IVF centers instead operate an on-site or near-site genetics laboratory, eliminating the courier leg entirely — this is the foundation of "rapid PGT-A" protocols discussed later.

Accessioning at the reference lab

On arrival, samples are accessioned: barcodes are scanned into the laboratory information system (LIS), tube integrity and labeling are verified against the requisition form, and any specimen with a discrepancy (missing label, temperature excursion, damaged tube) is flagged and the clinic is contacted before processing continues.

Accessioned samples then enter the processing queue for whole genome amplification — but they do not necessarily start immediately. Centralized labs batch multiple clinics' samples together to run cost-efficient, fully loaded sequencing runs, which is where the next major source of turnaround time is introduced.

Whole Genome Amplification & NGS Library Preparation

A handful of trophectoderm cells contain only picograms of DNA — far too little to sequence directly. Whole genome amplification multiplies this into microgram quantities, after which the DNA is converted into a barcoded sequencing library. Because both steps are run in batches for cost and quality-control efficiency, this is the stage where "waiting for a full run" most directly adds days to the timeline.

• ~30–60 pg: Starting DNA per sample (from 5–10 cells)
• ~1–2 µg: DNA after WGA (~30,000-fold amplification)
• 24–96: Typical batch size (samples per sequencing run)
• ~1 day: Library prep duration (fragmentation to indexing)

Whole genome amplification (WGA)

Multiple displacement amplification (MDA) or PCR-based WGA kits are used to amplify the entire genomic content of the few biopsied cells uniformly enough that every chromosome region remains proportionally represented — a critical requirement, since the whole point of downstream sequencing is to measure relative chromosome dosage. Uneven amplification bias is one of the main technical challenges of PGT-A and is controlled for with validated kits and quality thresholds (DNA yield, amplification uniformity metrics) before a sample is allowed to proceed.

Samples that fail WGA QC — too little DNA, contamination, or amplification failure — are flagged for repeat testing where possible, which can add several additional days to that specific sample's turnaround.

NGS library construction

Amplified DNA is enzymatically or mechanically fragmented into short pieces (~200–300 bp), end-repaired, and ligated to sequencing adapters that include a unique sample-specific barcode (index). This barcoding is what allows dozens to nearly a hundred patient samples to be physically pooled together and sequenced simultaneously on one flow cell, then computationally separated afterward by barcode.

Library quality (fragment size distribution, concentration) is checked before pooling, typically via automated electrophoresis and fluorometric quantification, then libraries are normalized to equal molar concentration so that every sample receives a comparable number of sequencing reads regardless of its individual yield.

Because low-pass whole-genome sequencing only needs enough reads to bin the genome into chromosome-arm-level windows (not high-depth variant calling), 24–96 samples can share a single sequencing run — a batch of 96 barcoded PGT-A libraries can be sequenced together for a fraction of the per-sample cost of running each individually.

The batch-size trade-off

Batching drives down the cost per embryo tested — a genetics lab wants a flow cell loaded close to capacity before committing an expensive sequencing run. But a fixed run schedule (for example, sequencing twice per week) means a sample that just misses a cut-off has to wait for the next batch to fill.

Larger target batch sizes generally mean the lab waits longer to accumulate enough samples before starting a run, adding to turnaround time; smaller batches start sooner but cost more per sample and are run more frequently. High-volume reference labs mitigate this with predictable, frequent run schedules (e.g., every Monday and Thursday) so that the maximum wait for any individual sample is bounded regardless of instantaneous queue size.

Sequencing Run — Flow Cell Loading & Data Generation

Pooled, barcoded libraries are loaded onto a single sequencing flow cell and read in parallel. This is a fixed-duration, high-throughput step: once the run starts, every sample in the batch — regardless of which clinic or patient it came from — finishes at the same time.

• ~2–4 M: Reads needed per sample (low-pass coverage)
• ~13–30h: Typical run duration (depends on platform/read length)
• up to 96: Samples per flow cell (barcode-multiplexed)
• ~1 Mb: Genome bin resolution (per analysis window)

Low-pass whole-genome sequencing, not high-depth sequencing

PGT-A does not require deep, base-by-base sequencing of the entire genome — it needs just enough reads, spread evenly across all 24 chromosome types (1–22, X, Y), to count how many reads fall into each genomic bin and detect deviations from the expected two-copy (diploid) dosage. This is called low-pass or shallow whole-genome sequencing, typically targeting only 0.01–0.1× genome coverage per sample.

Because the depth requirement per sample is so low, a single sequencing run can be divided — via barcoding — across dozens of samples simultaneously, which is the technical basis for the batch economics described in the previous stage.

Cluster generation and base calling

On the flow cell, each library molecule is clonally amplified into a small cluster of identical copies (bridge amplification or equivalent), producing enough fluorescent signal per cluster to be optically read. Sequencing-by-synthesis instruments then cycle through incorporation of fluorescently labeled bases, imaging the flow cell after each cycle, and calling the base incorporated at every cluster.

Modern short-read platforms complete this process — for a run configuration typical of PGT-A libraries — in roughly half a day to a day and a half depending on instrument, read length, and how full the flow cell is loaded. The run proceeds identically whether it is 50% or 100% full, which is why labs prefer to wait for a fuller batch: the fixed run time and reagent cost is amortized over more samples.

Once a sequencing run begins, its duration is essentially fixed by chemistry and instrument cycle time — filling more of the flow cell with samples changes cost-per-sample dramatically, but it does not meaningfully lengthen the run itself. The dominant lever on turnaround at this stage is how long the lab waited to start the run, not how long the run takes.

Demultiplexing

After the run completes, raw sequencing data is demultiplexed — sorted back into per-sample read files using each library's unique barcode — and basic run-level quality metrics (cluster density, Q30 base quality percentage, per-sample read yield) are reviewed before the data is released to the bioinformatics pipeline. A sample that received an unusually low read count due to library pooling imbalance may be flagged here for review or repeat sequencing.

Bioinformatics Pipeline & Copy Number Variant Calling

This is the fastest stage in the entire workflow — once sequencing data exists, an automated pipeline can turn raw reads into a chromosome-by-chromosome euploidy call within hours, not days. It is also the stage where the actual genetic information the clinic is waiting for is generated.

• ~2–8h: Pipeline runtime (per full batch)
• 24: Chromosomes assessed (1–22, X, Y)
• ~5–10 Mb: Aneuploidy detection resolution (segmental level)
• ~20–80%: Mosaicism detectable range (abnormal cell fraction)

From raw reads to a copy-number profile

Demultiplexed reads for each sample are aligned to the human reference genome, then the genome is divided into consecutive bins (roughly megabase-scale windows). The pipeline counts how many aligned reads fall into each bin, corrects for known biases (GC content, mappability, WGA amplification bias), and normalizes the result against a reference set of known-euploid samples.

A chromosome or chromosome segment present in the normal two copies will show a read-density ratio near 1.0 relative to baseline; a segment with three copies (trisomy) shows an elevated ratio near 1.5; a segment with one copy (monosomy) shows a reduced ratio near 0.5. The pipeline applies statistical segmentation algorithms (e.g., circular binary segmentation, hidden Markov models) to call the boundaries and copy-number state of every segment automatically.

Whole-chromosome, segmental, and mosaic calls

The automated caller classifies each embryo's result into categories such as:

• Euploid — all 24 chromosome types show normal copy number • Aneuploid — one or more whole chromosomes show a clear gain or loss (e.g., trisomy 21, monosomy X) • Segmental — a partial chromosome gain/loss below whole-chromosome scale, often ≥10 Mb to be reliably called • Mosaic — a mixed signal suggesting only a fraction of the biopsied cells carry the abnormality, reported as an estimated percentage range rather than a binary call

Because the biopsy samples only 5–10 cells out of several hundred in the trophectoderm, a mosaic result is an estimate of the abnormal cell fraction in that sample, not a certainty about the whole embryo — which is why mosaic results are typically flagged for additional genetic counseling before a transfer decision.

The bioinformatics stage itself typically finishes within a single working day of the sequencing run completing — often just a few hours for an automated pipeline to process a full batch. It is rarely the rate-limiting step in overall turnaround time; batching delays and human QC review upstream and downstream of it dominate the schedule.

Automated QC flags before human review

Before a case reaches the lab director, the pipeline itself applies automated quality gates: minimum read count per sample, noise/variance thresholds on the copy-number profile (a "noisy" low-quality profile can mimic mosaicism), and internal controls confirming the correct sample identity was maintained through WGA, library prep, and sequencing (barcode-to-sample concordance).

Samples that fail these automated checks are routed to a QC-hold queue rather than being auto-reported, ensuring that only technically adequate data reaches the human review stage next.

Lab Director QC Review, Report Delivery & FET Scheduling

No PGT-A result leaves the laboratory without a qualified lab director or clinical geneticist reviewing the copy-number plot for every embryo. This human review step is a regulatory and clinical-safety requirement — and once it is complete, the result travels through a secure reporting channel that ultimately determines when the patient's frozen embryo transfer can be booked.

• ~5–15 min: Manual review time (per embryo case)
• ~95–98%: Typical QC pass rate (of sequenced samples)
• 5–10: Total TAT, standard workflow (business days, biopsy → result)
• 24–48h: Total TAT, rapid on-site protocol (select high-volume centers)

Director-level sign-off

A board-certified laboratory director (or delegated qualified reviewer under applicable clinical laboratory regulations) manually inspects each embryo's copy-number plot: does the profile match a clean, confident call, or does it show noise, ambiguous segmental calls, or borderline mosaicism that needs a second reviewer or repeat analysis?

This step exists because automated CNV callers, while highly accurate on clean data, can be misled by technical artifacts (WGA bias, low input DNA, sample cross-contamination). Human oversight catches these edge cases before a result — which will directly influence which embryo is transferred — is released to a clinic.

Secure result delivery

Once signed off, the report is uploaded to a secure, access-controlled clinic portal (rather than emailed as a plain attachment) to protect protected health information, consistent with data-privacy regulations governing clinical genetic testing. The referring IVF clinic's embryology and physician team receives a notification, reviews the per-embryo results, and — together with the patient — selects which euploid (or otherwise suitable) embryo to prioritize for transfer.

From biopsy to a released report, the standard courier-and-batch workflow described across these five stages typically totals five to ten business days. Weekends, holidays, and repeat testing for failed or ambiguous samples can extend this further.

Scheduling the frozen embryo transfer

Because the embryo has been vitrified since biopsy, receiving the result does not itself create urgency for the embryo — but it does start the clock on scheduling. The patient's endometrium must be pharmacologically or naturally prepared for an FET cycle (typically 2–4 additional weeks of preparation once a euploid embryo is confirmed), so a faster genetics turnaround simply lets that preparation phase start sooner, compressing the overall time-to-pregnancy-attempt.

For patients and clinics, the practical value of a shorter PGT-A turnaround is almost entirely about scheduling velocity and reduced patient anxiety during the wait — not embryo safety, which is already secured by vitrification.

Rapid PGT-A and the fresh-transfer frontier

A small but growing number of high-volume centers operate on-site or near-site sequencing capability paired with streamlined, small-batch or single-sample bioinformatics pipelines, compressing the entire biopsy-to-report timeline to roughly 24–48 hours. Eliminating courier shipping and batch-queue waiting are the two biggest contributors to this compression — sequencing chemistry and human QC review times change comparatively little.

A sufficiently fast turnaround theoretically re-opens the possibility of a "fresh" (non-frozen) blastocyst transfer with PGT-A results in hand before the implantation window closes, rather than the freeze-all-and-wait model that dominates current practice. As of the mid-2020s this remains an emerging capability offered by a limited number of academic and high-throughput programs rather than the standard of care — most PGT-A cycles worldwide still rely on the centralized reference-lab batch workflow described in Stages 1–4, with vitrification as the default.

Standard vs. rapid on-site PGT-A workflow