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DAPI
DAPI
DAPI
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DAPI
Names
IUPAC name
2-(4-Amidinophenyl)-1H-indole-6-carboxamidine
Other names
4′,6-Diamidino-2-phenylindole
Identifiers
3D model (JSmol)
ChEBI
ChEMBL
ChemSpider
UNII
  • InChI=1S/C16H15N5/c17-15(18)10-3-1-9(2-4-10)13-7-11-5-6-12(16(19)20)8-14(11)21-13/h1-8,21H,(H3,17,18)(H3,19,20) checkY
    Key: FWBHETKCLVMNFS-UHFFFAOYSA-N checkY
  • InChI=1/C16H15N5/c17-15(18)10-3-1-9(2-4-10)13-7-11-5-6-12(16(19)20)8-14(11)21-13/h1-8,21H,(H3,17,18)(H3,19,20)
    Key: FWBHETKCLVMNFS-UHFFFAOYAH
  • [N@H]=C(N)c3ccc(c2cc1ccc(cc1[nH]2)C(=[N@H])N)cc3
  • [H]/N=C(/c1ccc(cc1)c2cc3ccc(cc3[nH]2)/C(=N/[H])/N)\N
Properties
C16H15N5
Molar mass 277.331 g·mol−1
Except where otherwise noted, data are given for materials in their standard state (at 25 °C [77 °F], 100 kPa).
checkY verify (what is checkY☒N ?)

DAPI (pronounced 'DAPPY', /ˈdæpiː/), or 4′,6-diamidino-2-phenylindole, is a fluorescent stain that binds strongly to adenine–thymine-rich regions in DNA. It is used extensively in fluorescence microscopy. As DAPI can pass through an intact cell membrane, it can be used to stain both live and fixed cells, though it passes through the membrane less efficiently in live cells and therefore provides a marker for membrane viability.

History

[edit]

DAPI was first synthesised in 1971 in the laboratory of Otto Dann as part of a search for drugs to treat trypanosomiasis. Although it was unsuccessful as a drug, further investigation indicated it bound strongly to DNA and became more fluorescent when bound. This led to its use in identifying mitochondrial DNA in ultracentrifugation in 1975, the first recorded use of DAPI as a fluorescent DNA stain.[1]

Strong fluorescence when bound to DNA led to the rapid adoption of DAPI for fluorescent staining of DNA for fluorescence microscopy. Its use for detecting DNA in plant, metazoa and bacteria cells and virus particles was demonstrated in the late 1970s, and quantitative staining of DNA inside cells was demonstrated in 1977. Use of DAPI as a DNA stain for flow cytometry was also demonstrated around this time.[1]

When bound to double-stranded DNA, DAPI has an absorption maximum at a wavelength of 358 nm (ultraviolet) and its emission maximum is at 461 nm (blue). Therefore, for fluorescence microscopy, DAPI is excited with ultraviolet light and is detected through a blue/cyan filter. The emission peak is fairly broad.[2] DAPI will also bind to RNA, though it is not as strongly fluorescent. Its emission shifts to around 500 nm when bound to RNA.[3][4]

DAPI (magenta) bound to the minor groove of DNA (green and blue). From PDB: 1D30​.

DAPI's blue emission is convenient for microscopists who wish to use multiple fluorescent stains in a single sample. There is some fluorescence overlap between DAPI and green-fluorescent molecules like fluorescein and green fluorescent protein (GFP) but the effect of this is small.

Outside of analytical fluorescence light microscopy DAPI is also popular for labeling of cell cultures to detect the DNA of contaminating Mycoplasma or virus. The labelled Mycoplasma or virus particles in the growth medium fluoresce once stained by DAPI making them easy to detect.[5]

Modelling of absorption and fluorescence properties

[edit]

This DNA fluorescent probe has been effectively modeled[6] using the time-dependent density functional theory, coupled with the IEF version of the polarizable continuum model. This quantum-mechanical modeling has rationalized the absorption and fluorescence behavior given by minor groove binding and intercalation in the DNA pocket, in term of a reduced structural flexibility and polarization.

Live cells and toxicity

[edit]

DAPI can be used for fixed cell staining. The concentration of DAPI needed for live cell staining is generally very high; it is rarely used for live cells.[7] It is labeled non-toxic in its MSDS[8] and though it was not shown to have mutagenicity to E. coli,[9] it is labelled as a known mutagen in manufacturer information.[2] As it is a small DNA binding compound, it is likely to have some carcinogenic effects and care should be taken in its handling and disposal.

Alternatives

[edit]
Endothelial cells stained with DAPI (blue), phalloidin (red) and through immunofluorescence via an antibody bound to fluorescein isothiocyanate (FITC) (green).

The Hoechst stains are similar to DAPI in that they are also blue-fluorescent DNA stains which are compatible with both live- and fixed-cell applications, as well as visible using the same equipment filter settings as for DAPI.

References

[edit]

See also

[edit]
Wikimedia Commons has media related to DAPI.
Revisions and contributorsEdit on WikipediaRead on Wikipedia

DAPI

View on Grokipedia
from Grokipedia
DAPI, or 4′,6-diamidino-2-phenylindole, is a synthetic, cell-permeable fluorescent dye that selectively binds to the minor groove of adenine-thymine (AT)-rich regions in double-stranded DNA, forming a highly fluorescent complex that enables visualization of cell nuclei and chromosomes under fluorescence microscopy. First synthesized in 1971 in the laboratory of Otto Dann at the University of Erlangen-Nuremberg as part of a program to develop diamidine-based drugs against trypanosomiasis, DAPI proved ineffective as an antiparasitic agent. Its fluorescent properties were first utilized in 1974 by Williamson and Fennell for isolating mitochondrial DNA, leading to its recognition as a DNA-specific fluorescent probe. Chemically, DAPI dihydrochloride ( C₁₆H₁₅N₅ · 2HCl; molecular weight 350.25) is a powder soluble in water (up to 20 mg/mL) but insoluble in , with excitation and emission wavelengths shifting upon DNA binding—from approximately 340 nm excitation and 453 nm emission in free form to 358 nm excitation and 461 nm emission in the DNA-bound state, respectively, typically observed in the blue spectrum. In biological research, DAPI is extensively employed for nuclear counterstaining in immunofluorescent assays, apoptosis detection via flow cytometry, mycoplasma contamination screening in cell cultures, and sensitive DNA visualization in agarose gels as an alternative to ethidium bromide, owing to its high specificity, low toxicity at working concentrations (typically 1–5 μg/mL), and ability to penetrate intact cell membranes for both live- and fixed-cell imaging. Its stability in aqueous solutions (lasting 2–3 weeks when protected from light and stored at 2–8°C) and compatibility with other fluorescent probes, such as those for cytoskeletal or labeling, have made DAPI a cornerstone tool in , , and since the 1970s.

Chemical Properties

Molecular Structure

DAPI, chemically known as 4',6-diamidino-2-phenylindole, has the molecular formula C16_{16}H15_{15}N5_5 in its form. The most commonly utilized variant is the dihydrochloride salt, with the formula C16_{16}H15_{15}N5_5·2HCl and a molecular weight of 350.25 g/mol, which offers enhanced solubility in aqueous media compared to the neutral . The molecular structure consists of a bicyclic core—a ring fused to a ring—with a phenyl attached at the 2-position of the and two groups (-C(=NH)NH2_2) positioned at the 4' site on the phenyl ring and the 6 site on the 's moiety. This arrangement forms a conjugated aromatic system, often described as having a biphenyl-like core due to the connected ring systems. The molecule lacks stereocenters and is achiral, exhibiting a predominantly planar conformation that facilitates its interactions in biological contexts. Crystal structures of DAPI-DNA complexes, such as the one in PDB entry 432D (d(GGCCAATTGG) at 1.9 Å resolution), reveal DAPI as a flat aromatic entity with slight deviations from perfect planarity. These structures show the coplanar orientation of the and phenyl rings, essential for the molecule's rigidity. The salt form is preferred in settings due to its superior (up to 20 mg/mL with heating) over the free base, which exhibits limited aqueous and often requires organic solvents like DMSO or for dissolution. This difference arises from the of the groups in the salt, increasing hydrophilicity.

Synthesis

The original synthesis of DAPI (4',6-diamidino-2-phenylindole) was reported by Dann et al. in 1971 as part of efforts to develop trypanosomicidal agents. Modern synthesis of DAPI and its analogues typically involves the protection of 5(6)-cyanoindoles, lithiation to form stannanes, Stille coupling with bromoaryl/heteroaryl benzonitriles to yield bisnitriles, and subsequent amidine formation using lithium bis(trimethylsilyl)amide followed by deprotection with ethanolic HCl. These methods provide good yields (e.g., 61-75%) and are used to explore antitrypanosomal activity and DNA binding properties. Purification of DAPI is commonly achieved through on using methanol-chloroform mixtures as eluents, followed by recrystallization from or to obtain the dihydrochloride salt. Characterization involves ^1H NMR spectroscopy to confirm the aromatic and protons, showing the molecular ion at m/z 278 for the , and determination of the dihydrochloride at >300°C (). These methods ensure high purity (>98%) suitable for applications.

Spectroscopic Properties

Absorption and Emission Spectra

DAPI in displays an absorption maximum at approximately 340 nm in the region and an emission maximum at 488 nm, characterized by a molar absorptivity (ε) of about 23,000 M⁻¹ cm⁻¹ at 342 nm. The of unbound DAPI remains low, typically around 0.02–0.04, reflecting its weak in free form due to efficient non-radiative decay pathways. This spectral profile positions DAPI as a UV-excitable probe suitable for fluorescence microscopy, though its inherent dimness limits utility without binding. Upon binding to double-stranded DNA, particularly in AT-rich regions, DAPI undergoes a red shift in its absorption spectrum to 358–364 nm, while the emission maximum blue-shifts to 454–461 nm. This interaction results in a dramatic 20-fold enhancement in fluorescence intensity, driven by an increase in quantum yield to about 0.6, alongside a Stokes shift of roughly 90–120 nm that facilitates effective separation of excitation and emission wavelengths in imaging applications. These changes underscore the probe's sensitivity to its microenvironment, with binding-induced rigidity suppressing quenching mechanisms. The spectral characteristics of DAPI are influenced by environmental factors, including solvent polarity and . In organic media such as , DAPI exhibits solvatochromic shifts, with higher quantum yields (up to 0.58) and altered emission profiles compared to aqueous conditions, highlighting its responsiveness to hydrophobic environments. is optimally observed at neutral values of 7–8, where protonation states favor DNA binding and emission efficiency; deviations, such as acidic conditions, can diminish intensity by altering the dye's charge and .

Fluorescence Mechanism

DAPI fluorescence arises from the absorption of (UV) photons by free DAPI at around 340 nm, which excites the molecule via a π-π* transition within its conjugated indolic and phenyl ring system. This process promotes an from the ground (S₀) to the lowest excited (S₁), as described in a simplified where to the (T₁) is minimal due to the molecule's structure. In the free state, rapid non-radiative decay from S₁ to S₀ predominates through vibrational relaxation and , resulting in weak with a of approximately 0.02. Upon binding to the minor groove of DNA, particularly in AT-rich regions, the fluorescence intensity increases dramatically, up to 20-fold (with absorption shifting to ~358 nm and emission to ~461 nm), due to the restriction of intramolecular rotations and torsional motions around the phenyl-indole bond. This binding enforces a more planar conformation of the DAPI molecule, reducing non-radiative quenching pathways such as twisted intramolecular charge transfer (TICT) and collisional deactivation. The apolar microenvironment of the DNA minor groove further stabilizes the excited state by limiting solvent interactions that promote deactivation in aqueous solution. Theoretical modeling using (TD-DFT) has elucidated the properties, revealing that the absorption energies are highly sensitive to the binding environment, while emission energies remain relatively consistent. Calculations indicate a HOMO-LUMO gap of approximately 3.5 eV for the free DAPI molecule, aligning with the observed UV absorption and corresponding to the energy of the π-π* transition. These models confirm that DNA binding alters the electronic distribution, with charge displacement toward the groups in the , enhancing radiative decay. Regarding photostability, DAPI undergoes photobleaching under prolonged UV excitation in microscopy, primarily through photoconversion and oxidative damage, with half-lives on the order of minutes under intense illumination conditions. For instance, significant bleaching occurs after 3 minutes of continuous UV exposure in standard setups, limiting prolonged imaging without antifade agents.

Simplified Jablonski Diagram for DAPI Fluorescence S₁ (π-π* excited state) ──→ Fluorescence emission (488 nm, free; ~461 nm bound) │ │ (Reduced non-radiative decay upon DNA binding) ▼ S₀ (Ground state) ←─── UV absorption (340 nm, free; ~358 nm bound) │ └─ Non-radiative decay (dominant in free DAPI)

Simplified Jablonski Diagram for DAPI Fluorescence S₁ (π-π* excited state) ──→ Fluorescence emission (488 nm, free; ~461 nm bound) │ │ (Reduced non-radiative decay upon DNA binding) ▼ S₀ (Ground state) ←─── UV absorption (340 nm, free; ~358 nm bound) │ └─ Non-radiative decay (dominant in free DAPI)

Biological Interactions

DNA Binding Specificity

DAPI binds to double-stranded DNA in a non-intercalative manner, primarily through minor groove binding in AT-rich regions of the B-DNA helix. This mode involves the insertion of the DAPI molecule into the narrow minor groove, where its positively charged amidine groups and heterocyclic rings interact with the DNA backbone and bases. Specifically, the indole NH group forms hydrogen bonds with the O2 atoms of thymine, while the amidine nitrogens establish bonds with the N3 atoms of adenine, stabilizing the complex through direct contacts with the floor of the groove. The binding affinity of DAPI is notably high for AT-rich sequences, with dissociation constants (K_d) typically in the range of 10–100 nM for sites containing consecutive AT base pairs, such as AATT. For example, the association constant (K_a) for the AATT site is reported as 5.5 × 10^8 M^{-1}, corresponding to a K_d of approximately 1.8 nM. DAPI shows a strong preference for poly(dA-dT) over GC-rich DNA, where groove binding is disfavored and intercalation occurs instead with lower affinity; this selectivity arises from the narrower and deeper minor groove in AT regions, accommodating the rigid structure of DAPI more effectively, with reported affinity ratios favoring AT sequences by factors of 10 to 1000 depending on the sequence context. In terms of , DAPI binds at a ratio of approximately one per 3–4 base pairs within AT-rich segments, as this spacing allows optimal accommodation in the minor groove without significant distortion. At higher concentrations or in longer AT tracts, binding exhibits positive , where adjacent DAPI molecules stabilize each other through hydrophobic stacking interactions between their aromatic rings, enhancing overall affinity and leading to clustered binding patterns. Structural evidence from confirms minor groove binding in the central AATT region and formation of direct hydrogen bonds to base atoms in the complex with the d(GGCCAATTGG)_2, where DAPI resides in the minor groove, displacing the hydration spine while the phenylindole moiety stacks parallel to the base pairs. Similar findings from NMR solution structures of DAPI bound to AT-containing duplexes, such as d(CGATTATTCG)_2, reveal a conformation of DAPI that fits snugly in the groove, underscoring the sequence-specific geometry.

Interaction with RNA and Proteins

DAPI exhibits weaker binding affinity to double-stranded RNA compared to DNA, with dissociation constants (Kd) typically in the range of 1–10 μM, primarily through intercalation rather than minor groove binding. This interaction results in a notable shift in the fluorescence emission spectrum to approximately 500 nm (green), as opposed to the blue emission (~450 nm) observed with DNA complexes, though the overall fluorescence intensity is substantially lower. Binding to single-stranded RNA is minimal, owing to the lack of stable helical structure required for effective intercalation, limiting non-specific RNA staining in most cellular assays. Interactions with proteins are generally of low affinity, driven by electrostatic attractions between DAPI's cationic amidine groups and negatively charged or basic residues in proteins. For instance, DAPI binds to basic proteins such as histones with modest strength, potentially contributing to background fluorescence in chromatin-rich environments, although the fluorescence enhancement is several-fold weaker than with DNA. This non-specific binding can occur via surface interactions on proteins like tubulins, where association constants reach ~2 × 10^5 M^{-1} (Kd ≈ 5 μM), but such complexes rarely interfere significantly with DNA-specific applications due to their low quantum yield. Comparative binding assays, including fluorescence titration and displacement studies, demonstrate DAPI's high selectivity for DNA under standard physiological conditions (e.g., 150 mM NaCl, pH 7.4), underscoring its utility despite minor off-target interactions with RNA and proteins.

Applications

In Fixed Cell Imaging

In fixed cell imaging, DAPI serves as a widely adopted nuclear counterstain due to its strong affinity for DNA in permeabilized samples, enabling clear visualization of nuclear morphology and facilitating colocalization studies with other cellular markers. A standard protocol begins with fixation of cells using 4% paraformaldehyde in phosphate-buffered saline (PBS) for 10-20 minutes at room temperature to preserve cellular architecture while maintaining DNA accessibility. This is followed by permeabilization with 0.1-0.3% Triton X-100 in PBS for 5-10 minutes, which disrupts the plasma and nuclear membranes to allow DAPI penetration without compromising structural integrity. Cells are then incubated with DAPI at 1 μg/mL in PBS for 5-10 minutes at room temperature, protected from light to prevent photodegradation, and washed three times with PBS to remove unbound dye. This step is commonly integrated with antibody counterstaining, where primary antibodies targeting proteins of interest are applied post-permeabilization, followed by fluorescent secondary antibodies before or after DAPI addition, enabling simultaneous detection in immunofluorescence assays. DAPI offers distinct advantages in fixed cell applications, including excellent tissue penetration after permeabilization and a stable fluorescent signal that withstands prolonged storage and repeated imaging sessions post-fixation. Its excitation at wavelengths (around 358 nm) and emission in the blue spectrum (461 nm) ensure minimal spectral overlap with green (e.g., FITC or GFP) or red fluorophores, supporting robust multicolor imaging without crosstalk. Protocol optimization is essential for achieving consistent results across sample types. For cultured cells, 1 μg/mL DAPI typically yields optimal nuclear intensity, while thicker tissue sections may require 2-5 μg/mL or extended incubation (up to 20 minutes) to compensate for diffusion barriers and ensure even staining depth. preservation during long-term is achieved by mounting samples in antifade media, such as glycerol-based formulations containing antioxidants like ProLong Gold, which reduce signal decay by inhibiting formation. Common artifacts in DAPI-stained fixed cells include overstaining, which can cause non-specific cytoplasmic due to excess binding to or proteins, or spectral bleed-over into adjacent channels, potentially masking colocalized signals. , manifested as rapid signal loss under excitation light, is mitigated by limiting UV exposure and using antifade mounting agents, ensuring reliable quantification of nuclear features over extended observation periods.

In Live Cell Imaging

DAPI's application in live cell imaging is limited by its poor membrane permeability, which prevents efficient entry into intact viable cells without additional interventions. Unlike in fixed samples, where DAPI readily accesses DNA, live cell protocols require modifications to facilitate delivery while preserving cell viability. This has led to its selective use in short-term studies where nuclear labeling is essential for tracking dynamic processes, though more permeable dyes like Hoechst 33342 are often preferred for routine live-cell nuclear staining. Protocol adaptations for live cell imaging typically involve either elevated DAPI concentrations or physical delivery methods to overcome membrane barriers. For direct incubation, concentrations of 5–10 μg/mL are used for 10–30 minutes to allow limited penetration, suitable for short-term imaging in permeable cell types. Alternatively, enables efficient intracellular delivery by creating transient pores in the plasma membrane, allowing DAPI to label nuclei in adherent cells for subsequent fluorescence microscopy; this method has been optimized for high efficiency with minimal viability loss in cell lines like U2OS. provides precise, localized introduction of DAPI directly into the or nucleus, particularly useful for single-cell studies in models like embryos, where it supports real-time visualization without widespread toxicity. These approaches contrast with standard fixed cell protocols by emphasizing rapid, low-dose application to avoid prolonged exposure. In live cell applications, DAPI facilitates analysis by binding DNA to reveal progression phases through nuclear intensity variations, often combined with for long-term tracking in setups. It also enables monitoring of nuclear dynamics, such as movements or envelope remodeling, via time-lapse ; low-intensity UV excitation is employed to capture these events while reducing photodamage and maintaining signal stability over minutes to hours. These techniques have been applied in studies of proliferation and regeneration, providing insights into real-time cellular behaviors. Key limitations include DAPI's exclusion from intact live cells, necessitating invasive delivery that can introduce artifacts or reduce viability, and its susceptibility to , where intensity fades over hours under repeated illumination, complicating extended sessions. Signal degradation is exacerbated in UV-sensitive setups, often requiring antifade additives or intermittent imaging to sustain nuclear visualization.

Toxicity and Safety

Cellular Toxicity

DAPI exerts cellular toxicity through its high-affinity binding to the minor groove of AT-rich DNA regions, which disrupts DNA-directed enzymatic processes involved in replication, transcription, and repair. This interference can lead to inhibition of DNA synthesis and RNA production, contributing to cell cycle arrest and eventual cell death in exposed cells. In mammalian cells, DAPI demonstrates dose-dependent . is significantly reduced in short-term exposures of less than 1 hour, where concentrations below 10 μM are generally tolerated, allowing brief use in live cell imaging without immediate cell loss. At higher concentrations (>10 μM), DAPI penetrates live cell membranes more effectively but induces prolonged effects, including reduced viability and morphological changes indicative of stress. In vivo studies in animal models have revealed limited data on genotoxic potential, with DAPI showing no mutagenic activity in the using typhimurium strains. To mitigate these effects, researchers often employ structural analogs like Hoechst 33342, which exhibit lower while maintaining similar DNA-binding properties, or opt for pulsed dosing in experimental protocols to limit accumulation. Suppliers such as Thermo Fisher issue warnings on product labels regarding potential cellular at working concentrations, recommending dilution and avoidance of prolonged contact with live cells.

Handling Precautions

DAPI, a fluorescent DNA-intercalating agent, presents specific physical and during handling, primarily due to its potential for dust generation and skin sensitization. As a fine , it poses an risk, necessitating the use of a or well-ventilated area to minimize airborne exposure. (PPE) is essential, including chemical-resistant gloves, safety goggles, and protective clothing to prevent and ; respiratory protection may be required if dust levels are high. The compound is light-sensitive and should be stored in the dark to maintain stability, with recommended conditions including refrigeration or freezing at -20°C in tightly sealed, original containers away from direct sunlight and heat sources. Under these conditions, DAPI powder typically has a of 1-2 years, while stock solutions remain for several months when protected from light and freeze-thaw cycles. Disposal of DAPI and contaminated materials must comply with local environmental regulations, treating it as due to its classification under the Globally Harmonized System (GHS) as skin irritation (Category 2), skin sensitization (Category 1A), and specific target organ toxicity - single exposure, irritation (Category 3). It should be collected by licensed waste contractors and never released into drains, sewers, or waterways. In the event of a spill, evacuate the area and ensure adequate ventilation before response; personnel should wear appropriate PPE as outlined above. Absorb the spill using inert materials such as or , place the collected material in sealed containers for disposal, and clean residues with water or a mild while preventing runoff into environmental systems.

History

Discovery and Development

DAPI, or 4',6-diamidino-2-phenylindole, was first synthesized in 1971 by Otto Dann and colleagues Gerhard Bergen, Ekke Demant, and Gerda Volz at the Institute of Pharmacology and Toxicology, University of Erlangen-Nuremberg, Germany. The compound emerged from a systematic research program aimed at developing novel diamidine derivatives as potential trypanocidal agents to combat trypanosomiasis, a parasitic disease caused by Trypanosoma species. Although DAPI exhibited limited efficacy as an antiparasitic drug, its strong binding affinity to DNA was noted during initial characterization, and its fluorescence properties were discovered in subsequent studies in 1975, paving the way for its repurposing as a biological probe. The synthesis and preliminary evaluation of DAPI were detailed in the seminal 1971 publication by Dann et al. in Justus Liebigs Annalen der Chemie, which described the preparation of various 2-phenylindole-based diamidines, including DAPI, along with their basic spectroscopic and biological properties. This work highlighted DAPI's ability to form fluorescent complexes with nucleic acids, though the focus remained on its potential therapeutic applications at the time. Early experiments revealed that DAPI binds preferentially to the minor groove of AT-rich DNA sequences, emitting blue fluorescence upon excitation at ultraviolet wavelengths, a property that distinguished it from other diamidines in the series. By 1975, just four years after its synthesis, DAPI's fluorescence capabilities led to its rapid adoption as a DNA-specific in biological . The first documented application was in microscopy for detecting contamination in cell cultures, as reported by Russell, Newman, and Williamson, who demonstrated DAPI's high sensitivity in visualizing extranuclear DNA from infecting mycoplasmas without significant background interference. Concurrently, Williamson and Fennell utilized DAPI to and separate yeast during cesium chloride ultracentrifugation, marking the initial recognition of its utility in distinguishing organellar DNA from nuclear DNA based on intensity and density gradients. These pioneering uses established DAPI as a versatile tool for visualization, shifting its development trajectory from toward cytochemistry and .

Key Milestones

Following its initial synthesis in 1971, DAPI was commercialized in the 1970s by Sigma-Aldrich, marking its entry into routine laboratory use as a fluorescent DNA stain. This availability facilitated broader adoption in molecular biology, with the dye now distributed by major suppliers such as Thermo Fisher Scientific, ensuring high-purity formulations for diverse applications. A seminal 1995 review by Kapuscinski detailed DAPI's binding properties and fluorescence characteristics, solidifying its role as a standard tool for DNA visualization and quantitation in histochemistry and flow cytometry. In the 1980s, DAPI saw significant integration with emerging techniques, as commercial confocal systems became available in the mid-decade, enabling high-resolution three-dimensional imaging of DAPI-stained nuclei in biological specimens. This adoption enhanced DAPI's utility in studying cellular structures, with early applications demonstrated in wavelength-optimized confocal setups for precise nuclear labeling. By the , DAPI was routinely incorporated as a in (FISH) protocols, supporting the technique's rapid expansion for mapping DNA sequences on chromosomes, as evidenced by combined DAPI-banding and FISH methods that allowed simultaneous detection of probe signals and patterns. The brought increased recognition of DAPI's cellular , particularly its interference with live-cell processes due to its binding to , prompting the development of handling guidelines in protocols to minimize exposure risks such as and respiratory . Safety data sheets and assay guidelines from this era emphasized its use primarily in fixed samples, influencing shifts toward less toxic alternatives for dynamic . In the , DAPI has been adapted for advanced applications, including visualization in CRISPR-based techniques like CRISPR-FISH, where it serves as a nuclear to map edited genomic loci with high specificity. Recent studies have explored nanoparticle-mediated delivery of DAPI for enhanced , improving cellular uptake and reducing toxicity in targeted applications such as confocal analysis of nanoparticle-labeled cells.

Alternatives

Structurally Similar Dyes

Among the dyes sharing analogous chemical scaffolds with DAPI, the Hoechst bisbenzimides, such as Hoechst 33258 and Hoechst 33342, stand out for their similar AT-specific minor groove binding to DNA. These dyes feature a bisbenzimide core that facilitates strong interactions with adenine-thymine rich sequences, much like DAPI's indole-based structure. Both exhibit excitation maxima around 350 nm and emission maxima near 460 nm, producing blue fluorescence upon DNA binding. Hoechst 33342, in particular, includes an ethyl group that enhances its lipophilicity compared to Hoechst 33258. In comparison to DAPI, Hoechst dyes demonstrate superior membrane permeability, allowing effective staining of live cells without fixation, whereas DAPI is primarily suited for fixed specimens due to its lower cell-permeant nature. DAPI, however, offers greater photostability, resisting bleaching better during prolonged imaging sessions. Hoechst dyes were originally developed by in the 1970s and remained under patent protection until the early , after which they became widely available as generic compounds. Selection between DAPI and Hoechst often hinges on toxicity profiles—Hoechst being less cytotoxic for live applications—and spectral compatibility with other fluorophores in multicolor experiments. Other structural analogs include DIPI [4′,6-bis(2-imidazolin-2-yl)-2-phenylindole], a derivative of DAPI featuring imidazoline rings instead of amidine groups that exhibits enhanced binding affinity to DNA, resulting in brighter fluorescence and negligible fading during chromosome banding analyses. Unlike the groove-binding mode of DAPI and Hoechst, ethidium bromide serves as an intercalating analog with a distinct phenanthridinium scaffold, inserting between base pairs and emitting red fluorescence (excitation ~300-510 nm, emission ~600 nm), though it is selected less frequently for cellular imaging owing to its higher mutagenicity. These dyes are chosen based on factors like toxicity—ethidium bromide requires stringent handling—and compatibility with UV or visible excitation sources.

Modern Substitutes

Modern substitutes for DAPI have emerged to mitigate its limitations, particularly in live-cell imaging where UV excitation can induce and . These contemporary DNA stains often operate in the far-red spectrum, enabling reduced cellular damage while maintaining high specificity for nuclear labeling. They facilitate with other fluorophores and support applications in without requiring cell fixation. Recent developments as of 2024 include far-red stains like NucSpot Far-Red Nuclear Stain, which provides selective nuclear labeling in fixed cells with near-IR emission for enhanced . SiR-DNA, a silicon-rhodamine-based far-red probe, serves as a low-toxicity alternative for live-cell nuclear imaging with an excitation wavelength around 650 nm. It exhibits high specificity for DNA, minimal background staining, and compatibility with super-resolution microscopy techniques. Developed for nanoscopy applications, SiR-DNA demonstrates negligible cytotoxicity in various cell types and tissues, allowing prolonged observation without significant impairment to cellular processes. DRAQ5 and DRAQ7 represent cell-permeant, far-red anthraquinone derivatives that provide non-toxic nuclear staining in live cells without the need for fixation. DRAQ5 rapidly labels DNA in both live and fixed samples, emitting in the far-red range for easy integration into multi-color assays. DRAQ7, similarly non-toxic even at concentrations up to 20 μM over 72 hours, is particularly valued for real-time viability assessments by selectively staining compromised cells while sparing healthy ones. Both dyes offer stable, stoichiometric binding to double-stranded DNA, supporting flow cytometry and imaging workflows. NucBlue Live ReadyProbes, introduced in the 2020s by , consists of an optimized Hoechst 33342 formulation in a ready-to-use dropper bottle for high-throughput nuclear in live cells. This commercial reagent reduces preparation time and UV exposure variability compared to traditional DAPI protocols, enabling efficient screening of apoptotic nuclear changes via blue fluorescence at 460 nm. It stains nuclei of all cells uniformly, with increased intensity over time in unfixed samples, and is validated for fluorescence microscopy in diverse cell lines. These substitutes offer key advantages over DAPI, including lower genotoxicity due to far-red excitation that minimizes DNA damage from UV light, and expanded spectral compatibility for multiplexing with green and red channels. Comparative studies confirm their equivalent efficacy in nuclear labeling, with SiR-DNA and DRAQ5 providing comparable specificity and signal intensity to DAPI in live-cell assays while exhibiting reduced phototoxicity. For instance, far-red probes like SiR-DNA enable less damaging imaging in sensitive multiplexing setups.

References

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