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Base Cat #A71071

EGFR Polyclonal Antibody

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Recognizes EGFR for research focused on kinase signaling and phosphorylation pathways.

We recommend using an alternative (Catalog #A79228): EGFR Monoclonal Antibody [8G4B1]
Application: IHCIPWB
Clonality: Polyclonal
Conjugate: Unconjugated
Host: Rabbit
Isotype: IgG
Purification: Affinity Purified
Reactivity: Human, Mouse, Rat
100% Guarantee: 6 months
Application Guarantee for AntibodiesRecombinant Rabbit Monoclonal Abs
Catalog No.SizePriceQty
A71071-100100 µl $299.00 
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Availability: Discontinued 

Product Overview

Background
The protein encoded by this gene is a transmembrane glycoprotein that is a member of the protein kinase superfamily. This protein is a receptor for members of the epidermal growth factor family. EGFR is a cell surface protein that binds to epidermal growth factor. Binding of the protein to a ligand induces receptor dimerization and tyrosine autophosphorylation and leads to cell proliferation. Mutations in this gene are associated with lung cancer.

Description
EGFR Polyclonal Antibody. Unconjugated. Raised in: Rabbit.

Formulation
Buffer: PBS with 0.02% sodium azide, 50% glycerol, pH7.3.

Specificity
Human, Mouse, Rat

Isotype
IgG

Uniprot ID
P00533

Purification
Affinity Purified

Immunogen
Recombinant fusion protein containing a sequence corresponding to amino acids 1021-1210 of human EGFR (NP_005219.2).

Storage
Shipped at 4°C. Upon receipt, store at -20°C. Avoid freeze / thaw cycles

Alternative Names
EGFR; ERBB; ERBB1; HER1; NISBD2; PIG61; mENA; epidermal growth factor receptor

Application
WB, IHC, IP; Recommended dilution: WB 1:500 - 1:2000, IHC 1:50 - 1:200, IP 1:50 - 1:100

Datasheet & SDS

PDF
Datasheet/User Guide: A71071 If the above file is not available online, you can request a copy by contacting us.

Applications

Suggested protocols for EGFR Polyclonal Antibody should be self-optimized according to the user's experiment.

Choose Your Experiment Type

Use this Western blot protocol guide to choose conditions for sample preparation, SDS-PAGE gel selection, protein transfer, membrane blocking, antibody incubation, detection, controls, and troubleshooting. Select the experiment type that best matches your sample or target, including routine lysate, recombinant protein, tagged protein, low-abundance target, small protein or histone, large protein, membrane protein, phospho/PTM target, IP-Western or pulldown eluate, or secreted protein.

Routine cell or tissue lysate Western blot protocol

For most 20-100 kDa targets in whole-cell lysate or tissue lysate.

  • Use this workflow when: You are detecting a typical 20-100 kDa target in whole-cell lysate, nuclear extract, cytoplasmic extract, or tissue lysate.
  • Optimize first: Sample quality, protein normalization, transfer consistency, antibody dilution, blocking buffer, and exposure time.

Before you start

  • Confirm the expected molecular weight and the antibody host species before starting.
  • Prepare fresh protease inhibitors in cold lysis buffer. For nuclear protein lysates, consider EpiQuik Nuclear Extraction Kit (OP-0002); for histone protein lysates, consider EpiQuik Total Histone Extraction Kit (OP-0006).
  • Plan 10-30 ug total protein per lane as the starting load.
  • Include a positive control, negative control when available, and a validated loading control or total protein stain.

Protocol

1Prepare and clarify the sample

  1. For cells, collect cells directly and wash with cold PBS when appropriate. For tissues, cut and homogenize tissue pieces, then collect and wash the resulting cell pellet.
  2. Lyse on ice in your own cold lysis buffer containing fresh protease inhibitors, or use the reference lysis buffer preparation below. For nuclear protein lysates, consider EpiQuik Nuclear Extraction Kit (OP-0002); for histone protein lysates, consider EpiQuik Total Histone Extraction Kit (OP-0006).
  3. Incubate on ice for 10-30 minutes with occasional mixing.
  4. Clarify at 12,000-16,000 x g for 10-20 minutes at 4°C.
  5. Transfer only the clear supernatant to a fresh tube. If lysate is viscous, shear DNA before loading.

2Quantify, normalize, and denature

  1. Measure protein concentration before adding reducing sample buffer.
  2. Normalize all samples to the same concentration.
  3. Add 4X Laemmli sample buffer to 1X final concentration.
  4. Heat at 95°C for 5 minutes, then briefly centrifuge before loading.

3Run SDS-PAGE

  1. Use a 10-12% gel or 4-12% gradient gel for most routine targets.
  2. Load ladder, positive control, negative control, and test samples.
  3. Run the stacking gel at 60-80 V, then the resolving gel at 100-150 V.
  4. Stop when the dye front approaches the bottom or the target range is separated.

4Transfer to membrane

  1. Use 0.45 um PVDF or nitrocellulose for routine targets.
  2. For wet transfer, start around 100 V for 60-90 minutes at 4°C, or use validated semi-dry settings.
  3. Stain the membrane with Ponceau S before blocking to confirm transfer and lane consistency.
  4. Correct uneven transfer before changing antibody conditions.

5Block, probe, detect, and normalize

  1. Block with 5% non-fat dry milk in TBST unless the antibody datasheet recommends another blocker.
  2. Incubate EGFR Polyclonal Antibody using the dilution, incubation time, and buffer recommended in the antibody datasheet or supplier specifications.
  3. Wash 3 x 5-10 minutes, incubate secondary antibody, then wash again.
  4. Capture non-saturated exposures and normalize to total protein or a validated loading control.

Controls to include

  • Positive lysate or purified protein that is known to contain the target.
  • Negative lysate, knockout, knockdown, untreated, or low-expression sample when available.
  • Loading control such as GAPDH, beta-actin, tubulin, or a total protein stain.
  • Short and long exposures to avoid relying on a saturated image.

Purified or recombinant protein Western blot protocol

For purified target protein, recombinant controls, standards, or defined protein preparations.

  • Use this workflow when: You are confirming expression, purity, identity, tag detection, or recovery of a purified or overexpressed recombinant protein.
  • Optimize first: Protein loading amount, tag or target antibody choice, gel percentage, transfer time, and exposure range.

Before you start

  • Use nanogram-range loading instead of total lysate loading ranges.
  • Prepare a dilution series so signal intensity can be interpreted without saturation.
  • Confirm the final expected size, including tag, linker, fusion partner, or cleavage product.
  • Include unrelated recombinant protein, buffer-only control, or tag-only control when relevant.

Protocol

1Prepare a dilution series

  1. Dilute the protein in compatible buffer before adding sample buffer.
  2. Start with 1-50 ng per lane for most purified proteins.
  3. Include at least three amounts, such as low, medium, and high load.
  4. Use a buffer-only lane if the storage buffer contains reducing agent, salt, glycerol, detergent, or carrier protein.

2Denature without overloading

  1. Add 4X sample buffer to 1X final concentration.
  2. Heat at 95°C for 5 minutes unless the protein aggregates.
  3. If precipitation appears after heating, test 37-70°C for 10-30 minutes.
  4. Briefly centrifuge before loading.

3Run SDS-PAGE by final protein size

  1. Choose gel percentage by the final expected recombinant protein size.
  2. Use a gradient gel if expected contaminants or fragments span a wide molecular weight range.
  3. Run the gel until the target and any expected fragments are separated.
  4. Do not interpret an overloaded purified lane as antibody specificity.

4Transfer

  1. Use 0.45 um membrane for most recombinant proteins above about 20 kDa.
  2. Use 0.2/0.22 um membrane for very small proteins or peptides.
  3. Confirm transfer with Ponceau S or another reversible stain.
  4. If signal is too intense, reduce protein load before changing transfer conditions.

5Probe and interpret

  1. Start with datasheet antibody dilution or a small antibody titration.
  2. Capture exposure times that keep the dilution series within the non-saturated range.
  3. Use unrelated recombinant protein or tag-only protein to check non-specific recognition.
  4. Use lysate validation separately if the antibody will be used on complex samples.

Controls to include

  • Purified target protein as the main positive control.
  • Unrelated recombinant protein to check non-specific recognition.
  • Tag-only control if the detection antibody recognizes a tag.
  • Buffer-only lane to identify artifacts from storage buffer.

Tagged protein expression Western blot protocol

For FLAG, HA, His, Myc, GFP, or other tagged proteins expressed in cells or host lysates.

  • Use this workflow when: You are detecting HA, FLAG, His, Myc, GFP, or another tagged construct in transfected, transduced, or engineered samples.
  • Optimize first: Tag accessibility, expression level, lysis conditions, positive and mock-transfected controls, and antibody dilution.

Before you start

  • Calculate the final expected molecular weight, including tag, linker, fusion partner, and cleavage site.
  • Prepare matched samples such as transfected vs mock, induced vs uninduced, or expression vector vs empty vector.
  • Select lysis conditions based on tagged protein localization. For tagged nuclear proteins, consider EpiQuik Nuclear Extraction Kit (OP-0002); for tagged histone proteins, consider EpiQuik Total Histone Extraction Kit (OP-0006).
  • Use anti-tag antibody to confirm expression and target-specific antibody to confirm identity when possible.
  • Plan lower lysate loads if expression is very strong.

Protocol

1Prepare matched expression lysates

  1. Collect test and control samples under the same lysis conditions.
  2. Lyse on ice in your own cold lysis buffer containing fresh protease inhibitors, or use the reference lysis buffer preparation below. For nuclear protein lysates, consider EpiQuik Nuclear Extraction Kit (OP-0002); for histone protein lysates, consider EpiQuik Total Histone Extraction Kit (OP-0006).
  3. Centrifuge lysates at 12,000-16,000 x g for 10-20 minutes at 4°C.
  4. Start with 10-30 ug total protein per lane, or less if overexpression is strong.
  5. Keep induced/uninduced or transfected/mock samples paired on the same gel.

2Normalize and denature

  1. Quantify protein and normalize all lysates.
  2. Add reducing sample buffer to 1X final concentration.
  3. Heat at 95°C for 5 minutes unless the tagged protein aggregates.
  4. If the protein smears or remains in the well, test lower-temperature denaturation.

3Run gel by final tagged size

  1. Choose gel percentage based on the final construct size, not the native protein alone.
  2. Use 10-12% gel for many 25-100 kDa constructs, higher percentage for small tags, and lower percentage for large fusions.
  3. Run the gel long enough to separate full-length target from degradation products.
  4. Use an appropriate molecular weight ladder covering the full construct size.

4Transfer

  1. Transfer based on final target size.
  2. Use 0.45 um membrane for most tagged proteins above about 20 kDa.
  3. Check transfer before blocking.
  4. If the target is a large fusion protein, use large-protein transfer settings.

5Probe with tag and target logic

  1. Probe with anti-tag antibody to confirm expression.
  2. Probe with target-specific antibody when identity needs confirmation.
  3. Compare signal against mock, empty-vector, or uninduced control.
  4. If anti-tag gives many bands, reduce load and check for degradation.

Controls to include

  • Mock or untransfected lysate to identify host-cell background.
  • Empty-vector lysate to control for tag-related signal.
  • Induced and uninduced samples for inducible expression systems.
  • Target-specific antibody confirmation when anti-tag signal alone is not enough.

Low-abundance endogenous target Western blot protocol

For weak endogenous targets, rare proteins, inducible proteins, or targets that are difficult to detect in total lysate.

  • Use this workflow when: The target is weak, rare, inducible, tissue-restricted, or expected to produce a low signal in routine lysate.
  • Optimize first: Positive control choice, sample enrichment, protein load, EGFR Polyclonal Antibody incubation, wash stringency, and exposure time.

Before you start

  • Identify a strong positive control before running unknown samples.
  • Consider enrichment, IP, fractionation, nuclear extraction, or membrane enrichment instead of simply loading more lysate.
  • Use fresh inhibitors and keep samples cold.
  • Plan overnight EGFR Polyclonal Antibody incubation and sensitive detection.

Protocol

1Prepare or enrich the target

  1. Use total lysate only if the target is expected to be detectable without enrichment.
  2. For nuclear, membrane, chromatin-associated, or low-copy targets, enrich the appropriate fraction first. For nuclear protein enrichment, consider EpiQuik Nuclear Extraction Kit (OP-0002).
  3. Start with 20-40 ug total lysate only if lane quality remains acceptable.
  4. Include the positive control on the same blot.

2Normalize and denature

  1. Quantify protein or normalize enriched fraction by a consistent basis.
  2. Add reducing sample buffer and heat at 95°C for 5 minutes unless the target requires another condition.
  3. Avoid overloading total lysate because it can increase background faster than target signal.
  4. Clarify again if samples become viscous or particulate.

3Run SDS-PAGE

  1. Choose gel percentage by target size.
  2. Avoid distorted lanes, since weak targets become harder to interpret in smeared samples.
  3. Run the target region with enough separation from abundant nearby proteins.
  4. Do not compensate for low abundance by overloading until enrichment has been considered.

4Transfer and check before probing

  1. Use transfer settings based on target size.
  2. Stain the membrane after transfer and document the target molecular weight region.
  3. If the positive control is weak, troubleshoot transfer before antibody dilution.
  4. For small or large low-abundance targets, use the matching small- or large-protein transfer approach.

5Increase detection sensitivity in order

  1. Use overnight primary incubation at 4°C.
  2. Use a sensitive ECL or fluorescent detection reagent.
  3. Increase EGFR Polyclonal Antibody concentration only after confirming transfer and positive control.
  4. Avoid increasing secondary antibody first if background is already present.

Controls to include

  • Strong known positive control to confirm the assay can detect the target.
  • No-primary or secondary-only control if background is a concern.
  • Fraction marker or enrichment control if enrichment is used.
  • Loading control or total protein stain suited to the fraction or sample type.

Small protein, histone, or peptide Western blot protocol

For histones, peptides, small cytokines, and proteins below about 20 kDa.

  • Use this workflow when: The target is a small protein, histone, peptide-sized target, or low molecular weight modification-sensitive protein.
  • Optimize first: High-percentage gel selection, membrane pore size, transfer time, methanol level, and prevention of over-transfer.

Before you start

  • Use a high-percentage gel or Tris-Tricine gel for small target resolution.
  • Prepare 0.2/0.22 um membrane to reduce blow-through.
  • Use lower sample loads for abundant histones. For histone extraction from mammalian cells or tissues, consider EpiQuik Total Histone Extraction Kit (OP-0006).
  • Plan total H3, total H4, total histone, peptide, or recombinant control when appropriate.

Protocol

1Prepare the small-protein sample

  1. Use histone extract, enriched fraction, purified peptide, or total lysate depending on the target.
  2. For histone extracts, start around 0.5-5 ug per lane.
  3. For total lysate small targets, use the lowest load that still gives visible target signal.
  4. Avoid excessive loading because small abundant proteins can saturate quickly.

2Denature

  1. Add sample buffer to 1X final concentration.
  2. Heat at 95°C for 5 minutes unless the antibody or sample type requires another condition.
  3. Briefly centrifuge before loading.
  4. Keep peptide or histone controls prepared consistently with samples.

3Run a small-protein gel

  1. Use 15-18% gel or Tris-Tricine gel for very small targets.
  2. Run until the small target is separated from the dye front and nearby bands.
  3. Use a ladder that covers low molecular weight markers.
  4. If small bands compress, change gel chemistry before changing antibody conditions.

4Transfer gently

  1. Use 0.2/0.22 um PVDF or nitrocellulose.
  2. Use shorter or gentler transfer than routine proteins.
  3. Avoid SDS in transfer buffer unless specifically validated.
  4. If signal is missing, check for membrane blow-through before increasing antibody.

5Block, probe, and normalize

  1. Use blocker compatible with the antibody. For many histone PTM antibodies, start with BSA in TBST.
  2. Probe with target or modification-specific antibody.
  3. Normalize histone targets to total H3/H4, total histone, or total protein signal when appropriate.
  4. Use short exposures first because histone signals can saturate.

Controls to include

  • Total H3, total H4, or total histone control for histone targets.
  • Modified peptide, recombinant histone, or known positive sample for PTM targets.
  • Unmodified peptide or untreated sample when testing modification specificity.
  • Transfer retention check because small proteins can pass through membranes.

Large protein Western blot protocol

For proteins above about 150 kDa, high molecular weight targets, or proteins that transfer poorly.

  • Use this workflow when: The target is a large protein that transfers slowly or resolves poorly on a standard gel.
  • Optimize first: Gel percentage, transfer time, membrane choice, sample denaturation, and reducing conditions.

Before you start

  • Use a low-percentage or gradient gel suitable for high molecular weight separation.
  • Plan wet transfer with cooling and longer transfer time.
  • Prepare reduced-methanol transfer buffer when needed.
  • Plan membrane stain and post-transfer gel stain to check whether protein remains in the gel.

Protocol

1Prepare clean lysate

  1. Lyse on ice and avoid harsh handling that promotes aggregation.
  2. Clarify thoroughly before loading.
  3. Start with 10-30 ug total protein per lane depending on target abundance.
  4. Avoid viscous or particulate samples, which can trap large proteins near the well.

2Denature with care

  1. Use reducing sample buffer unless non-reducing conditions are required.
  2. Start with 95°C for 5 minutes for routine large soluble proteins.
  3. If the protein aggregates or stays near the well, test 37-70°C for 10-30 minutes.
  4. Briefly centrifuge before loading.

3Run a large-protein gel

  1. Use 4-8% gel or 4-15% gradient gel depending on target size.
  2. Run longer at appropriate voltage to improve high molecular weight separation.
  3. Use a high molecular weight ladder.
  4. If the target remains compressed near the top, lower the gel percentage before changing antibody conditions.

4Use extended wet transfer

  1. Use wet transfer with cooling instead of a short routine transfer.
  2. Start with 30 V overnight or another validated extended wet-transfer condition.
  3. Reduce methanol to 5-10% if large protein transfer is poor.
  4. Consider 0.025-0.05% SDS only after optimizing methanol and transfer time.

5Probe and check transfer first

  1. Block with milk or datasheet-recommended blocker.
  2. Use antibody conditions from the datasheet when available.
  3. If signal is weak, stain the post-transfer gel to determine whether target remained in the gel.
  4. Optimize transfer before increasing antibody concentration.

Controls to include

  • High molecular weight ladder.
  • Known positive lysate for the large target.
  • Ponceau S or total protein stain on membrane.
  • Post-transfer gel stain when transfer efficiency is uncertain.

Membrane or hydrophobic protein Western blot protocol

For membrane-enriched, hydrophobic, multi-pass, organelle, or detergent-sensitive proteins.

  • Use this workflow when: The target is hydrophobic, multi-pass, poorly soluble, or found mainly in membrane fractions.
  • Optimize first: Lysis buffer detergents, sample heating conditions, membrane fraction enrichment, gel percentage, and transfer efficiency.

Before you start

  • Choose lysis or extraction conditions strong enough to solubilize the target.
  • Prepare membrane fraction and cytosolic marker controls when fractionation is used.
  • Plan a denaturation comparison if boiling may cause aggregation.
  • Confirm detergent compatibility with SDS-PAGE and antibody detection.

Protocol

1Extract the membrane target

  1. Use detergent conditions appropriate for the membrane protein and sample type.
  2. Keep samples cold and include fresh inhibitors.
  3. Clarify insoluble debris after extraction.
  4. If fractionating, keep membrane and cytosolic fractions clearly separated.

2Normalize and test denaturation

  1. Normalize by protein concentration or fraction-equivalent loading.
  2. Start with standard reducing sample buffer.
  3. If boiling causes aggregation, test 37-70°C for 10-30 minutes.
  4. Avoid repeated freeze-thaw cycles, which can worsen aggregation.

3Run SDS-PAGE

  1. Choose gel percentage by target size.
  2. Watch for material remaining in the well or broad smearing.
  3. If migration is poor, optimize extraction and denaturation before changing antibody conditions.
  4. Use fraction marker lanes when possible.

4Transfer

  1. Use transfer settings based on target size.
  2. Use 0.45 um membrane for most membrane proteins above about 20 kDa.
  3. Check transfer before blocking.
  4. Optimize transfer only after sample solubilization is acceptable.

5Probe and reduce background

  1. Start with datasheet-recommended blocker or 5% milk in TBST for routine targets.
  2. Increase wash stringency if hydrophobic samples create broad background.
  3. Confirm signal is enriched in the membrane fraction when fractionation is used.
  4. If target is weak, troubleshoot extraction before increasing secondary antibody.

Controls to include

  • Membrane fraction marker to confirm enrichment.
  • Cytosolic marker to check fraction purity.
  • Positive membrane-rich sample.
  • No-primary control if hydrophobic background is high.

Phospho-specific or labile PTM Western blot protocol

For phosphorylation or other modification-specific targets that require careful sample handling and controls.

  • Use this workflow when: You are detecting phosphorylation, acetylation, methylation, ubiquitination, or another modification-specific target.
  • Optimize first: Inhibitor protection, treatment controls, blocking buffer, antibody specificity controls, and non-saturated exposure.

Before you start

  • Add phosphatase and protease inhibitors fresh to lysis buffer.
  • Keep samples cold and process quickly.
  • Use BSA in TBST as the starting blocker unless the antibody datasheet recommends otherwise.
  • Prepare total target, stimulated/unstimulated, inhibitor-treated, or phosphatase-treated controls when possible.

Protocol

1Lyse quickly with inhibitors

  1. Chill samples, tubes, and buffer before lysis.
  2. Add inhibitors immediately before use.
  3. Lyse and clarify samples at 4°C.
  4. Avoid delays, repeated freeze-thaw cycles, and prolonged handling.

2Normalize and denature

  1. Quantify protein and normalize all samples.
  2. Add sample buffer promptly after lysis.
  3. Heat at 95°C for 5 minutes unless the antibody datasheet recommends another condition.
  4. Keep the handling time consistent across treatment groups.

3Run SDS-PAGE

  1. Choose gel percentage by the total target protein size.
  2. Use better-resolving conditions if a modification-dependent mobility shift is expected.
  3. Run treated and untreated samples together.
  4. Avoid overloading, which can obscure subtle PTM-dependent changes.

4Transfer

  1. Transfer based on target size and confirm transfer before probing.
  2. Use membrane stain to verify consistent lane transfer.
  3. If phospho signal is weak, confirm total target before increasing phospho antibody.
  4. Use small- or large-protein transfer settings if target size requires them.

5Block, probe, and confirm specificity

  1. Block and dilute antibody in 3-5% BSA in TBST unless datasheet recommends otherwise.
  2. Probe phospho/PTM signal and total target protein.
  3. Confirm signal changes with stimulation, inhibition, or phosphatase treatment when possible.
  4. Switch blocker before assuming the antibody failed if background is high.

Controls to include

  • Total target protein to confirm expression and loading.
  • Stimulated and unstimulated samples to show expected modification change.
  • Phosphatase-treated sample when applicable.
  • Pathway inhibitor or treatment control when applicable.

IP, co-IP, or pulldown Western blot protocol

For IP-Western analysis of immunoprecipitated, co-IP, pulldown, bead-bound, or enriched eluate samples. This Western blot workflow assumes the IP or pulldown capture step has already been performed.

  • Use this workflow when: The immunoprecipitation, co-IP, pulldown, or enrichment step has already been performed and the eluate or bead-bound fraction will be analyzed by Western blot.
  • Optimize first: Input and IgG controls, heavy-chain and light-chain interference, elution method, sample loading, and detection antibody strategy.

Before you start

  • Plan lane order before starting: input, flow-through, wash, eluate, IgG IP, and beads-only when possible.
  • Check whether the target overlaps IgG heavy chain near 50 kDa or light chain near 25 kDa.
  • Choose a detection strategy that avoids IP antibody chain interference when needed.
  • Keep input and control samples for interpretation.

Protocol

1Collect IP fractions

  1. Save input before IP.
  2. Save flow-through and wash fractions if capture efficiency matters.
  3. Elute target from beads under conditions compatible with downstream Western blotting.
  4. Include IgG IP and beads-only control when possible.

2Prepare eluate for loading

  1. Add sample buffer to eluate or bead-bound sample according to the IP method.
  2. Boil beads in sample buffer only if compatible with the experiment.
  3. Briefly centrifuge and load the supernatant without bead carryover.
  4. Load input as a small percentage of starting material and eluate as an equivalent fraction.

3Run SDS-PAGE

  1. Choose gel percentage by target size.
  2. Account for IgG heavy chain near 50 kDa and light chain near 25 kDa.
  3. If the target overlaps IgG chains, use detection designed to avoid chain interference.
  4. Separate input, control IP, and test IP lanes clearly.

4Transfer

  1. Use transfer settings based on target size.
  2. Confirm transfer before blocking.
  3. If sample amount is limited, avoid unnecessary membrane stripping.
  4. Use small- or large-target transfer changes only when target size requires them.

5Probe and interpret enrichment

  1. Use light-chain-specific, conformation-specific, or directly conjugated detection if IgG chain interference is expected.
  2. Compare test IP to IgG IP and beads-only control.
  3. Use input to confirm that the target was present before IP.
  4. Troubleshoot enrichment before assuming Western blot antibody failure.

Controls to include

  • Input to show the target was present before IP.
  • Flow-through and wash to evaluate capture and wash loss.
  • IgG IP to measure non-specific antibody pulldown.
  • Beads-only IP to measure non-specific bead binding.

Secreted protein or conditioned media Western blot protocol

For conditioned media, culture supernatant, serum-containing media, or concentrated secreted protein samples.

  • Use this workflow when: The target is secreted into conditioned media, serum-free media, plasma, serum, or another low-protein extracellular sample.
  • Optimize first: Sample concentration, matrix background, loading normalization, positive controls, and transfer/detection sensitivity.

Before you start

  • Clarify media to remove cells and debris before concentration or loading.
  • Choose a normalization basis: volume, cell number, viability, total protein, or another experiment-specific factor.
  • Concentrate media if the target is expected to be dilute.
  • Include blank media and conditioned-media positive control when possible.

Protocol

1Clarify and normalize media

  1. Centrifuge conditioned media to remove cells and debris.
  2. Concentrate the media if target abundance is low.
  3. Normalize by volume, cell number, viability, total protein, or collection time.
  4. Record the normalization basis so lanes can be compared.

2Prepare sample buffer

  1. Add sample buffer after concentration or cleanup.
  2. Use reducing or non-reducing conditions based on the target and antibody.
  3. If concentrated media contains high salt, desalt or clean up before loading.
  4. Avoid overloading serum proteins if serum-containing media is used.

3Run SDS-PAGE

  1. Choose gel percentage by target size.
  2. Run blank media, conditioned media, and positive control on the same gel.
  3. If serum proteins dominate the lane, reduce load or use serum-free collection when feasible.
  4. If migration is distorted, check salt and concentration method.

4Transfer

  1. Transfer based on target size.
  2. Use 0.45 um membrane for most routine secreted proteins above about 20 kDa.
  3. Confirm transfer with membrane stain.
  4. If target is small, use small-protein transfer settings.

5Probe and compare to media controls

  1. Block with datasheet-recommended blocker or 5% milk for routine targets.
  2. Increase washing if serum or media components create background.
  3. Compare conditioned media against blank media control.
  4. Use viability data to distinguish secretion from protein release due to cell death.

Controls to include

  • Blank media to identify media-derived background.
  • Conditioned-media positive control or purified target.
  • Cell viability control to help distinguish secretion from cell lysis.
  • Normalization record for volume, cell number, viability, or protein basis.
Open full WB protocol

Choose Your IHC Workflow

Use this immunohistochemistry protocol guide to run antibody staining in FFPE tissue, frozen tissue, fluorescent tissue staining, or optimization workflows.

FFPE chromogenic IHC protocol

Use this workflow for formalin-fixed paraffin-embedded tissue stained with HRP/DAB or another chromogenic detection system.

  • Use this format when: Evaluating protein expression or localization in FFPE tissue sections by brightfield microscopy.
  • Optimize first: Antigen retrieval buffer, retrieval time, primary antibody dilution, blocking, detection chemistry, and hematoxylin counterstain.
1
Bake and deparaffinize slides
Bake 4-5 um FFPE sections at 60 degrees C for 30-60 minutes. Deparaffinize in xylene, 2 changes for 5 minutes each. Rehydrate through 100 percent, 95 percent, and 70 percent ethanol, 2-3 minutes each, then rinse in water.
2
Perform antigen retrieval
Place slides in citrate buffer pH 6.0 or Tris-EDTA buffer pH 9.0. Heat near boiling for 10-20 minutes using a pressure cooker, microwave, steamer, or water bath. Cool slides in buffer for 20 minutes, then rinse in TBS or PBS.
3
Block endogenous activity
For HRP detection, incubate slides in 3 percent hydrogen peroxide for 10 minutes to quench endogenous peroxidase. Rinse 3 times in buffer.
4
Block nonspecific binding
Apply protein block, 5 percent normal serum, or 1-5 percent BSA for 20-60 minutes at room temperature. Drain but do not rinse if the detection system recommends leaving blocking protein on the section.
5
Add primary antibody
Dilute EGFR Polyclonal Antibody in antibody diluent. Start with the datasheet-recommended IHC dilution or test 1:50, 1:100, 1:250, and 1:500. Apply 100-200 uL per section and incubate 1 hour at room temperature or overnight at 4 degrees C in a humidified chamber.
6
Wash after primary antibody
Wash 3 times for 5 minutes each in TBS-T or PBS-T. Keep slides covered with buffer and do not let tissue dry.
7
Apply secondary or polymer detection
Apply HRP polymer, biotinylated secondary plus streptavidin-HRP, or another detection reagent according to the system instructions. Typical incubation is 20-30 minutes at room temperature. Wash 3 times.
8
Develop chromogen
Apply DAB or other chromogen for 1-10 minutes while monitoring signal under a microscope. Stop development by rinsing in water.
9
Counterstain and mount
Counterstain with hematoxylin for 15 seconds to 2 minutes, blue in running tap water or bluing reagent, dehydrate through ethanol, clear in xylene, and mount with permanent mounting medium.
Retrieval optimizationIf signal is weak, compare pH 6 and pH 9 retrieval before dramatically increasing antibody concentration.
Negative controlUse no-primary, isotype control when appropriate, and known negative tissue to evaluate nonspecific staining.

Frozen tissue IHC protocol

Use this workflow for frozen sections when antigen preservation is more important than FFPE morphology.

  • Use this format when: The epitope is fixation-sensitive, lipid-rich tissue is used, or frozen-section staining is preferred.
  • Optimize first: Fixation method, section thickness, drying time, blocking, primary antibody dilution, and tissue autofluorescence or endogenous enzyme activity.
1
Prepare frozen sections
Cut 5-10 um cryosections and mount onto charged slides. Air dry 10-30 minutes at room temperature. Store slides cold if staining later.
2
Fix sections
Fix with cold acetone for 10 minutes at -20 degrees C, cold methanol for 5-10 minutes, or 4 percent paraformaldehyde for 10-15 minutes depending on the target. Rinse gently in PBS or TBS.
3
Block endogenous activity if needed
For HRP-based detection, quench endogenous peroxidase with 0.3-3 percent hydrogen peroxide for 10 minutes. For biotin-based detection, consider avidin/biotin blocking when tissue has high endogenous biotin.
4
Block nonspecific binding
Block 20-60 minutes with 5 percent normal serum or 1-5 percent BSA in PBS/TBS. Use serum from the secondary antibody host species when practical.
5
Add primary antibody
Dilute EGFR Polyclonal Antibody in antibody diluent. Start with the datasheet-recommended frozen IHC dilution or test 1:50 to 1:500. Apply 100-200 uL per section and incubate 1 hour at room temperature or overnight at 4 degrees C.
6
Wash and detect
Wash 3 times for 5 minutes. Apply secondary antibody, polymer detection, or fluorescent secondary antibody according to the detection system. Incubate 30-60 minutes.
7
Develop or mount
For chromogenic detection, apply substrate until signal develops, rinse, counterstain, and mount. For fluorescent detection, protect from light, counterstain with DAPI if needed, and mount with antifade medium.
MorphologyFrozen sections usually preserve antigenicity better but morphology can be less crisp than FFPE tissue.
Section adhesionUse charged slides and avoid harsh washing if sections lift from the slide.

Fluorescent IHC protocol

Use this workflow for fluorescent staining of tissue sections when colocalization or multiplex imaging is needed.

  • Use this format when: Tissue localization is needed with fluorescent readout, multiple markers, or confocal microscopy.
  • Optimize first: Autofluorescence control, antigen retrieval, fluorophore choice, antibody host species, and mounting medium.
1
Prepare and retrieve tissue
For FFPE tissue, deparaffinize, rehydrate, and perform antigen retrieval. For frozen tissue, fix according to target requirements. Rinse in PBS or TBS.
2
Reduce autofluorescence
Treat autofluorescent tissues with a compatible quenching reagent when needed. Avoid quenchers that interfere with the planned fluorophores.
3
Permeabilize and block
Use 0.1-0.3 percent Triton X-100 for intracellular access when compatible. Block with 5 percent normal serum or 1-5 percent BSA for 30-60 minutes.
4
Add primary antibody
Dilute EGFR Polyclonal Antibody in blocking buffer. Start with the datasheet-recommended IHC/IF dilution or test 1:100, 1:250, and 1:500. Apply 100-200 uL per section and incubate 1-2 hours at room temperature or overnight at 4 degrees C.
5
Wash and add fluorescent secondary
Wash 3 times for 5 minutes. Add cross-adsorbed fluorescent secondary antibody at 1:500-1:1000 for 45-60 minutes protected from light.
6
Counterstain and mount
Wash 3 times. Add DAPI if desired. Mount with antifade medium and coverslip without bubbles.
7
Image and control
Acquire no-primary, single-color, and full-stain controls. Use identical image settings for samples that will be compared.
Multiplex tissue stainingFor multiple primary antibodies, confirm species compatibility or use directly conjugated primaries or sequential staining.
AutofluorescenceTissue autofluorescence can resemble true signal. Always compare to no-primary controls.

IHC optimization protocol

Use this workflow when an antibody or tissue type needs condition screening before final staining.

  • Use this format when: Signal is weak, background is high, staining is inconsistent, or the antibody is being validated in a new tissue.
  • Optimize first: Positive tissue, retrieval pH, antibody dilution, incubation time, detection strength, and blocking strategy.
1
Choose control tissue
Use a known positive tissue or cell pellet and a known negative tissue when available. Include the experimental tissue only after positive control staining is working.
2
Build a retrieval matrix
Test no retrieval, citrate pH 6.0, and Tris-EDTA pH 9.0 when tissue availability allows. Use the same section thickness and slide type for all conditions.
3
Test antibody dilution
Dilute EGFR Polyclonal Antibody across a small matrix such as 1:50, 1:100, 1:250, and 1:500, or follow datasheet starting ranges. Keep retrieval and detection constant while testing dilution.
4
Compare incubation conditions
If signal is weak, compare 1 hour at room temperature with overnight at 4 degrees C. Longer incubation can improve weak signal but may increase background.
5
Adjust detection strength
If signal remains weak, increase polymer incubation within the detection system limits, use amplification, or extend chromogen development while monitoring background.
6
Reduce background
Increase wash time, reduce antibody concentration, change blocking buffer, shorten chromogen development, or add detergent to wash buffer if compatible with the tissue and detection system.
7
Lock the protocol
Once the best condition is chosen, stain all comparative samples together using the same retrieval, antibody dilution, incubation time, detection system, and development time.
One change at a timeChange one major variable at a time when troubleshooting so the cause of improvement is clear.
DocumentationRecord lot numbers, retrieval buffer, heating method, antibody dilution, incubation time, detection system, and imaging settings.
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Choose Your IP Workflow

Use this immunoprecipitation protocol guide to enrich a target protein, preserve protein complexes, handle crosslinked samples, or perform RNA immunoprecipitation using antibody-based capture.

Protein immunoprecipitation protocol

Use this workflow to enrich a target protein from cell or tissue lysate using an antibody and protein A/G magnetic or agarose beads.

  • Use this format when: Pulling down a target protein for Western blot, mass spectrometry, enzymatic assay, or interaction analysis.
  • Optimize first: Lysis buffer stringency, lysate amount, antibody amount, bead amount, binding time, wash stringency, and elution method.
1
Prepare cold lysis buffer
Use your own non-denaturing IP-compatible lysis buffer or a buffer selected from the Western blot protocol that matches the sample type and target. As a starting point, use 20-50 mM Tris or HEPES pH 7.4-7.6, 150 mM NaCl, 1 percent NP-40 or Triton X-100, 1 mM EDTA, and fresh protease inhibitors such as Protease Inhibitor Cocktail when compatible with the downstream assay. Add phosphatase inhibitors for phospho or PTM targets.
2
Lyse sample
Use 0.5-2 mg total protein per IP as a starting range. Lyse cells on ice with cold lysis buffer containing fresh protease inhibitors. Incubate 15-30 minutes on ice with periodic mixing. For tissue, homogenize gently in cold lysis buffer. Clarify lysate at 12,000-16,000 x g for 10-15 minutes at 4 degrees C.
3
Pre-clear lysate
Add 20-30 uL washed protein A/G beads per IP to lysate and rotate 30-60 minutes at 4 degrees C. Collect supernatant and discard pre-clear beads to reduce nonspecific binding.
4
Bind antibody to target
Add 2-5 ug EGFR Polyclonal Antibody per 0.5-1 mg lysate as a starting point, or follow the datasheet. Rotate 2-4 hours at 4 degrees C, or overnight for low-abundance targets.
5
Capture immune complexes
Add 20-40 uL washed protein A/G magnetic or agarose beads per IP. Rotate 1-2 hours at 4 degrees C. Use protein A, protein G, or A/G according to antibody species and isotype.
6
Wash beads
Wash beads 3-5 times with 0.5-1 mL cold lysis buffer. For high background, add one higher-salt wash such as 300-500 mM NaCl if the interaction or epitope can tolerate it. Keep beads cold and minimize bead loss.
7
Elute target
For Western blot, add 20-40 uL 1x or 2x SDS sample buffer and heat 70-95 degrees C for 5-10 minutes depending on target stability and bead type. For native elution, use low pH glycine or competing peptide if compatible.
8
Analyze eluate
Run input, flow-through if needed, wash control, IgG control, beads-only control, and IP eluate. For WB detection, use a secondary antibody strategy that minimizes IgG heavy-chain and light-chain interference.
Antibody compatibilityWB validation does not guarantee IP performance. IP requires antibody binding under native or partially native conditions.
Heavy chain interferenceUse crosslinked antibody beads, light-chain-specific secondary antibody, native elution, or antibodies from different species when heavy chain overlaps the target size.

Co-IP protocol

Use this workflow to preserve and test protein-protein interactions during immunoprecipitation.

  • Use this format when: Pulling down a bait protein and detecting associated partner proteins.
  • Optimize first: Mild lysis conditions, salt concentration, detergent choice, lysate freshness, wash stringency, and reciprocal IP controls.
1
Use mild lysis conditions
Prepare cold mild lysis buffer such as 20-50 mM Tris or HEPES, 100-150 mM NaCl, 0.2-0.5 percent NP-40 or digitonin, 1 mM EDTA, and fresh inhibitors. Avoid harsh detergents and high salt unless the interaction is strong.
2
Lyse gently
Use fresh cells when possible. Lyse on ice for 15-30 minutes with gentle mixing. Clarify lysate at 10,000-14,000 x g for 10 minutes at 4 degrees C. Avoid sonication unless necessary because it can disrupt complexes.
3
Pre-clear
Pre-clear lysate with 20-30 uL beads for 30-60 minutes at 4 degrees C. Transfer the supernatant to a new tube.
4
Add bait antibody
Add 2-5 ug EGFR Polyclonal Antibody per IP if it is the bait antibody. Rotate 2-4 hours at 4 degrees C. For weak interactions, overnight incubation can help but may increase nonspecific binding.
5
Capture complexes
Add 20-40 uL protein A/G beads and rotate 1-2 hours at 4 degrees C. Keep all steps cold.
6
Wash gently
Wash 3-4 times with mild lysis buffer. If nonspecific bands are high, increase salt stepwise to 200-300 mM NaCl or reduce detergent exposure based on complex stability.
7
Elute and detect
Elute with SDS sample buffer for Western blot. Detect bait and suspected partner proteins on separate blots or after stripping when appropriate.
8
Confirm interaction
Include IgG control, beads-only control, input lysate, and reciprocal Co-IP when possible. Validate that the partner signal is enriched in the bait IP compared with controls.
Complex preservationCo-IP success depends heavily on keeping the complex intact. Use fresh lysate, cold buffers, and mild washing first.
Nuclease optionFor DNA- or RNA-mediated associations, add nuclease controls when needed to distinguish direct protein interaction from nucleic-acid bridged association.

Crosslinked IP or chromatin-associated target protocol

Use this workflow as a general crosslinked IP starting point for chromatin-associated proteins. For full ChIP workflows, see the dedicated ChIP protocol.

  • Use this format when: A chromatin-associated protein or complex needs crosslink-stabilized enrichment before downstream analysis.
  • Optimize first: Crosslinking time, chromatin fragmentation, antibody amount, wash stringency, reversal conditions, and DNA/protein recovery method.
  • Alternative workflow: If the goal is target-specific protein-DNA enrichment rather than conventional crosslinked IP or ChIP, consider EpiNext CUT&LUNCH Assay Kit or EpiNext CUT&RUN-Fast Kit.
1
Crosslink sample
Treat cells with 1 percent formaldehyde for 10 minutes at room temperature as a starting condition. Quench with 125 mM glycine for 5 minutes. Wash cells with cold PBS containing inhibitors.
2
Prepare nuclei or lysate
Collect cells and prepare nuclei or chromatin-enriched lysate using a compatible buffer. Keep samples cold and include protease inhibitors.
3
Fragment chromatin or complexes
Sonicate or digest to produce the fragment size needed for the downstream assay. For ChIP-qPCR, 200-800 bp DNA fragments are often used. Confirm shearing before large experiments.
4
Clarify and pre-clear
Clarify lysate and pre-clear with blocked protein A/G or ChIP-compatible beads for 30-60 minutes at 4 degrees C.
5
Add antibody
Add 2-10 ug EGFR Polyclonal Antibody per IP depending on target abundance and chromatin amount. Rotate overnight at 4 degrees C for chromatin-associated targets.
6
Capture and wash
Add blocked beads and rotate 1-2 hours. Wash sequentially with low-salt, high-salt, LiCl or detergent wash, and TE buffer when compatible with the downstream method.
7
Elute and reverse crosslinks
Elute complexes and reverse crosslinks, commonly at 65 degrees C for 2-6 hours or overnight depending on protocol. Treat with RNase and proteinase K if recovering DNA.
8
Purify and analyze
Purify DNA or protein as required. Analyze by qPCR, sequencing library preparation, Western blot, or other downstream method.
Dedicated ChIP pageFor optimized native and crosslinking ChIP details, see the dedicated ChIP protocol.
CrosslinkingOver-crosslinking can reduce antibody access and recovery. Start with mild crosslinking and optimize.
CUT&LUNCH or CUT&RUN-Fast optionFor protein-DNA interaction profiling from cells or tissues, use EpiNext CUT&LUNCH Assay Kit or EpiNext CUT&RUN-Fast Kit only when that assay format fits the experimental goal.

RNA immunoprecipitation protocol

Use this workflow to enrich RNA-associated proteins or protein-bound RNA while preserving RNA integrity.

  • Use this format when: Studying RNA-binding proteins, protein-RNA complexes, or RNA associated with a target protein.
  • Optimize first: RNase-free handling, lysis conditions, antibody amount, salt concentration, wash stringency, and RNA purification.
  • Kit option: For a complete RIP workflow with coordinated reagents, use EpiNext CUT&LUNCH RNA Immunoprecipitation (RIP) Kit when its sample type and downstream readout match the experiment.
1
Prepare RNase-free workspace
Use RNase-free tubes, filter tips, buffers, and gloves. Add RNase inhibitor to lysis, wash, and binding buffers when compatible.
2
Lyse cells gently
Lyse cells in RIP lysis buffer containing mild detergent, physiological salt, protease inhibitors, and RNase inhibitor. Use fresh lysate when possible. Clarify at 12,000-16,000 x g for 10 minutes at 4 degrees C.
3
Pre-clear lysate
Pre-clear lysate with washed beads for 30-60 minutes at 4 degrees C. Transfer supernatant to a new RNase-free tube.
4
Add antibody
Add 2-10 ug EGFR Polyclonal Antibody per RIP depending on target abundance. Rotate 2-4 hours or overnight at 4 degrees C. Include IgG control and input RNA controls.
5
Capture complexes
Add 20-40 uL protein A/G beads that have been washed and blocked with BSA, yeast tRNA, or other compatible blocking reagent. Rotate 1-2 hours at 4 degrees C.
6
Wash under RNase-free conditions
Wash 4-6 times with cold RIP wash buffer. Increase salt only if nonspecific RNA background is high and the interaction can tolerate it.
7
Recover RNA
Digest protein or reverse crosslinks if used, then purify RNA using phenol/chloroform, column purification, or magnetic bead cleanup. Include DNase treatment when downstream qPCR could detect DNA contamination.
8
Analyze RNA
Analyze enriched RNA by RT-qPCR, sequencing, or other downstream assay. Normalize to input and compare to IgG control.
RNase controlRNA loss is often caused by RNase contamination. Use RNase inhibitor and work quickly on ice.
Input controlSave 1-10 percent input before IP for normalization.
RIP kit optionFor a kit-based RNA immunoprecipitation workflow, consider EpiNext CUT&LUNCH RNA Immunoprecipitation (RIP) Kit when a complete RIP reagent set is preferred.
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