ACS Publications. Most Trusted. Most Cited. Most Read
DNA Sensing with Whispering Gallery Mode Microlasers
My Activity
  • Open Access
Letter

DNA Sensing with Whispering Gallery Mode Microlasers
Click to copy article linkArticle link copied!

  • Soraya Caixeiro*
    Soraya Caixeiro
    Department of Chemistry and Biochemistry, Humboldt Centre for Nano- and Biophotonics, Institute for Light and Matter, Greinstrasse 4-6, 50939 Cologne, Germany
    Centre for Photonics and Photonic Materials, Department of Physics, University of Bath, Bath BA2 7AY, United Kingdom
    *[email protected]
  • Robert Dörrenhaus
    Robert Dörrenhaus
    Department of Chemistry and Biochemistry, Institute of Organic Chemistry, Greinstrasse 4, 50939 Cologne, Germany
  • Anna Popczyk
    Anna Popczyk
    Department of Chemistry and Biochemistry, Humboldt Centre for Nano- and Biophotonics, Institute for Light and Matter, Greinstrasse 4-6, 50939 Cologne, Germany
    More by Anna Popczyk
  • Marcel Schubert
    Marcel Schubert
    Department of Chemistry and Biochemistry, Humboldt Centre for Nano- and Biophotonics, Institute for Light and Matter, Greinstrasse 4-6, 50939 Cologne, Germany
  • Stephanie Kath-Schorr*
    Stephanie Kath-Schorr
    Department of Chemistry and Biochemistry, Institute of Organic Chemistry, Greinstrasse 4, 50939 Cologne, Germany
    *[email protected]
  • Malte C. Gather*
    Malte C. Gather
    Department of Chemistry and Biochemistry, Humboldt Centre for Nano- and Biophotonics, Institute for Light and Matter, Greinstrasse 4-6, 50939 Cologne, Germany
    Centre of Biophotonics, SUPA School of Physics and Astronomy, University of St Andrews, St Andrews KY16 9SS, United Kingdom
    *[email protected]
Open PDFSupporting Information (1)

Nano Letters

Cite this: Nano Lett. 2025, 25, 11, 4467–4475
Click to copy citationCitation copied!
https://doi.org/10.1021/acs.nanolett.5c00078
Published March 4, 2025

Copyright © 2025 The Authors. Published by American Chemical Society. This publication is licensed under

CC-BY 4.0 .

Abstract

Click to copy section linkSection link copied!

Nucleic acid sensing is crucial for advancing diagnostics, therapeutic monitoring, and molecular biology research by enabling the precise identification of DNA and RNA interactions. Here, we present an innovative sensing platform based on DNA-functionalized whispering gallery mode (WGM) microlasers. By correlating spectral shifts in laser emission to changes in the refractive index, we demonstrate real-time detection of DNA hybridization and structural changes. The addition of gold nanoparticles to the DNA strands significantly enhances sensitivity, and exclusively labeling the sensing strand or a hairpin strand eliminates the need for secondary labeling of the target strand. We further show that ionic strength influences DNA compactness, and we introduce a hairpin-based system as a dual-purpose sensor and controlled release mechanism for drug delivery. This versatile WGM-based platform offers promise for sequence-specific nucleic acid sensing, multiplexed detection, and in vivo applications in diagnostics and cellular research.

This publication is licensed under

CC-BY 4.0 .
  • cc licence
  • by licence
Copyright © 2025 The Authors. Published by American Chemical Society

Nucleic acid chemistry is a fast-growing field with major implications for diagnostic and therapeutic applications as well as materials science. (1−3) A comprehensive understanding of the structure and dynamics of DNA and RNA is essential for a better understanding of their functions and for deeper insight into their mechanisms of action. (4) In addition to the formation of double-stranded DNA helices, the diverse folding of RNA or single-stranded DNA (ssDNA) and the dynamic changes in their structures under different conditions are essential for the function of nucleic acids. (5−7) In particular, oligonucleotide-based sensors are an expanding field of research and have proven to be a groundbreaking tool for prognosis and diagnosis. (8−14)

Lasers are well suited for enhancing the sensitivity of a wide range of measurements, primarily due to their narrow emission spectra resulting from stimulated emission. These properties are sometimes overlooked, and lasers are often used simply as a bright, directed, and narrow band excitation source for various applications, including excitation of fluorescence, Raman, surface plasmon resonance, and others. Instead, lasers can also be employed as sensors in their own right, (15−17) e.g., when their spectrum is used as a highly accurate external spectral ruler that shifts (18,19) and changes in intensity (20−22) through interaction of the laser with an analyte. This variant of laser-based sensing benefits considerably from the ability to make microscopic (volume of ≪50 μm3), low-cost, robust, and biocompatible lasers. In this context, the use of whispering gallery mode (WGM) lasers is particularly attractive. WGM lasers often operate by optical pumping of dye molecules embedded in an otherwise transparent microsphere, made, for instance, of polystyrene, and rely on the optical confinement of the resulting emission inside the microsphere due to a refractive index (RI) contrast with the environment. Over the past decade, there has been a quickly growing body of work where such lasers have been directly integrated with biological matter, e.g., for tracking of cell migration (23−25) and sensing cellular forces, (26,27) the latter even including noncontact measurements of local contractility in the living heart. (19) Looking at laser-based DNA sensing, double-stranded DNA (dsDNA) intercalated with a fluorescent dye has been employed both as a laser gain medium (28) and as a sensing conduit, with sensing activated through staining after the DNA is hybridized, a process that occurs only when the base pairs between the strands match. (29)

Gold nanoparticles (Au NPs) have a wide range of applications in optics, catalysis, biomedicine, and sensing, owing to their controllable physiochemical properties, high chemical stability, good biocompatibility, and excellent accessibility by wide-ranging surface functionalization. (30−32) These unique characteristics make Au NPs valuable for sensing applications involving variations in interactions between nanoparticles with differences in parameters such as particle type, shape, relative position, and number of particles (33,34) or even by assembling Au NPs with DNA to build complex structures with target-tailored functionalities. (35,36) Polystyrene microspheres coated with Au NPs have been used to sense viral DNA using a fluorescently labeled single-stranded (ssDNA) capture oligonucleotide; this method relies on a fluorescently labeled ssDNA capture oligonucleotide, where fluorescence quenching occurs upon hybridization with the target DNA. (8)

Beyond fluorescence-based sensing, Au NPs have also been used to locally enhance the electric field, therby improving WGM-based detection of DNA. (37−39) Their ability to concentrate electromagnetic fields at the nanoscale enhances optical signals, increasing the sensitivity of the biosensors. Over the past few decades, techniques for detecting short oligonucleotide sequences through in situ hybridization have expanded considerably. (8,40−42)

Here, to gain insight into the structure and dynamics of oligonucleotides, we developed a novel method for sensing structural changes in DNA immobilized on a WGM microlaser that uses the minute local variation in RI caused by these structural changes. This approach exploits the unique optical properties of WGM microlasers and their ability to measure external RI. We further enhance the sensitivity of our measurement by the addition of Au NPs to the DNA, which allows for the specific sensing of short DNA fragments.

In the example used in this study, the probe is based on a green-emitting, polystyrene-based WGM microlaser that is functionalized with ssDNA. Our model system consists of complementary strand DNA (csDNA) strands and DNA hairpin-forming strands. The polystyrene microlaser is covalently bound via a short linker to the strained cyclooctyne (SCO)-PEG3--modified 3′-end of an ssDNA sequence, which is modified with an amino group on its 5′-end and bound to a 2.2 nm diameter Au NP. Hybridization with csDNA leads to an increase of the RI in the immediate vicinity of the microlaser. This increase can be detected reliably through ensemble experiments on multiple lasers or via live analysis of an individual laser; the latter also provides insights into the hybridization dynamics. Moreover, we have developed a test system for a cleavable hairpin-based carrier that releases its Au NP only after the detection of specific DNA fragments.

In the future, with further investigation, our method could be adapted to detect the dynamics of ssDNA folding or to indicate hybridization or denaturation under different conditions. Our platform is highly versatile and can be adapted to detect different sequences of interest. Taken together, these characteristics make DNA-functionalized WGM lasers valuable tools for various applications in DNA sensing and analysis.

The WGM microlasers used in this study are commercially available, monodisperse fluorescent polystyrene (PS) microspheres, approximately 11 μm in diameter, featuring carboxyl groups on their surface for functionalization with ssDNA, and containing a green-emitting fluorescent dye dispersed within the PS matrix. The DNA sequences used are provided in Table S1. In brief, these sequences consist of a 22-base sequence modified at the 5′-end with an amine group for coupling to the carboxyl groups on the WGM microlasers or on Au NPs. Modifications at the 3′-end varied; some sequences were left unmodified, while others were conjugated with SCO-PEG3 for Au NP attachment or tagged with Cy5 dye for conjugation confirmation (see Figure S1).

Carboxyl groups on both the microlasers and the Au NPs were activated using carbodiimide chemistry, facilitating the formation of amide bonds with the amine-modified DNA. To prevent nonspecific binding, ethanolamine was used to block unreacted carboxyl groups. The DNA was then conjugated either to the Au NPs or directly to the microlasers.

To conjugate Au NPs, the Au NPs were covalently bound to the amino modification on the DNA’s 5′-end and the microlasers were first modified with 11-azido-3,6,9-trioxaundecan-1-amine, allowing the strain-promoted alkyne azide cycloaddition reaction (SPAAC) with the SCO-PEG3-terminated modified DNA, as described in the section 2 of the Supporting Information and illustrated in Figure 1a.

Figure 1

Figure 1. Preparation and optical characterization of the surface coating with gold nanoparticle (Au NP)-functionalized DNA on microlasers. (a) Schematic of the nanoparticle ssDNA conjugation to a carboxyl-functionalized microlaser. (b) Electron microscopy image of a carboxyl-functionalized microlaser. The scale bar is 2 μm. (c) Electron microscopy image of a microlaser decorated with DNA functionalized with 40 nm diameter Au NPs. Scale bars are 2 μm and 500 nm (inset). (e) Green fluorescence from a microlaser functionalized with ssDNA with Cy5 dye. (f) Red fluorescence of same microlaser. (g) Overlay of green and red emission. (h–j) Microlaser with dye-free ssDNA on the surface showing no red fluorescence (h). The hybridization with csDNA containing Cy5 illustrated in panel i leads to the appearance of a red ring in the fluorescence image (j). Scale bars for panels e–h and j are 20 μm.

To confirm successful modification of the microlaser surfaces with ssDNA, ssDNA tagged with the fluorescent dye Cy5 at its 3′-end was conjugated to the microlaser surface. Cy5 was selected for its red emission, which is well-separated from the absorption and emission spectra of the microlasers. Panels e–g of Figure 1 show the green fluorescence from the microlasers, the red fluorescence from ssDNA conjugated to its surface, and an overlay of the two images, respectively. The clearly visible fluorescent ring at the microlaser surface confirms the successful conjugation of ssDNA.

To confirm the modification of ssDNA strands with Au NPs and their subsequent attachment to the microlasers, we used 40 nm diameter Au NPs. This size was chosen for its ease of visualization using scanning electron microscopy (SEM), as detailed in section 2.6 of the Supporting Information. (Due to their small size and resolution limitations, 2.2 nm Au NPs were not visible via SEM, as shown in Figure S2.) All subsequent work used Au NPs with a diameter of 2.2 nm to avoid influencing DNA folding by NPs that are large compared to the DNA duplexes used, which have a calculated length of 6.6 nm for B-DNA duplexes. Figure 1b shows an SEM image of the smooth surface of an unmodified, carboxylated microlaser, while Figure 1c depicts a microlaser surface decorated with ssDNA conjugated with 40 nm Au NPs; a further magnified image is provided in Figure S3.

As further evidence for successful NP functionalization, we look at the addition of ssDNA conjugated with 40 nm Au NPs to a solution of azide-modified microlasers. Initially, the solution appeared red (Figure 1d, left tube) due to the plasmon resonance of the Au NPs dispersed in the solution. After 3 h, most of the NP-conjugated ssDNA has reacted with the microlasers, which precipitated to the bottom of the container due to their size and weight. As a result, the solution became nearly transparent (Figure 1d, right tube).

Lastly, csDNA was introduced, matching the sequence of ssDNA conjugated to the microlaser surface. To confirm conjugation, microlasers previously modified with the ssDNA were reacted with csDNA that was conjugated with Cy5 on its 3′-end (Figure 1i). While microlasers conjugated with ssDNA alone showed minimal red fluorescence (Figure 1h), there was a distinct ring-like emission on the surface after reaction with csDNA (Figure 1j), confirming successful hybridization to dsDNA.

The fluorescent molecules embedded within the PS microspheres can provide optical gain. When pumped with pulsed laser light above a threshold energy density of approximately 125 μJ/cm2, as established by previous studies, (18) the microspheres therefore emit laser light, and their emission spectra are dominated by a series of WGM lasing peaks. The emission spectrum of the lasers is characterized by a series of sharp peaks associated with alternating transverse-electric (TE) and transverse-magnetic (TM) modes, where the electric field of the light in the WGM is oriented either parallel (TE) or perpendicular (TM) to the surface. The exact wavelength of these peaks strongly depends on both the microlaser size and the RI in the immediate vicinity of the laser. A typical experimentally observed lasing spectrum is shown in Figure 2a. Panels b and c of Figure 2 show simulated emission spectra for a microlaser embedded in two media with different RIs (details on how these spectra were generated can be found in section 2.7 of the Supporting Information). For the medium with a higher RI, a red-shift in the positions of all peaks/modes is observed. By carefully analyzing the modal positions and knowing the internal RI of the microlaser, we were able to determine both the microlaser size and the external RI, following a routine described, e.g., in ref (43). Using this approach, the external RI for the microlaser in Figure 2a is determined to be 1.339.

Figure 2

Figure 2. Refractive index sensing of DNA surface modifications. (a) Representative lasing spectra from a microlaser in a buffered solution, along with the fitted refractive index. (b) Simulated lasing spectra for microlasers embedded in media of two different refractive indices: n = 1.340 (orange), and n = 1.345 (blue). (c) Close-up of the simulated spectra, highlighting the spectral shifts across different refractive indices and polarization, for azimuthal mode number m = 105. Histograms of external refractive indices calculated from measured laser spectra, with a corresponding box plot, showing (d) carboxyl-functionalized microlasers (N = 71), (e) microlasers conjugated with ssDNA (N = 99), (f) microlasers conjugated with dsDNA (N = 90), (g) microlasers conjugated with ssDNA and Au NPs (N = 65), and (h) microlasers conjugated with dsDNA and Au NPs (N = 91). The illustrations to the right of each histogram depict the configuration for each case.

Panels d–h of Figure 2 summarize the external RI for N > 40 microlasers for each successive step of surface functionalization, measured in the same buffered solution, clearly demonstrating a trend of increasing RI. As expected, the carboxylated microlasers exhibit the lowest external RI (Figure 2d), serving as the baseline for later modifications. Upon addition of ssDNA, we observe a modest increase in the mean external RI of just 0.0013 RIU, slightly smaller than the standard deviation of the mean, which is around 0.002 RIU and not statistically significant (Figure 2e). Similarly, the transition from ssDNA to helical B-form dsDNA through hybridization does not produce a statistically significant change in the RI (Figure 2f), suggesting that the structural alterations associated with hybridization are not captured within the resolution limit of the ensemble measurement.

A more pronounced effect is observed when ssDNA is conjugated with Au NPs at the 5′-end; in this scenario, the RI increases by 0.004 RIU (Figure 2g) compared to ssDNA without Au NPs and by 0.005 RIU compared to the bare carboxylated microlasers, resulting in statistically significant differences in RI distributions (p < 0.05). The larger standard deviation of 0.004 RIU likely reflects increased sample heterogeneity.

Compared to our initial experiment with unmodified DNA, the RI change from ssDNA-Au NPs to dsDNA-Au NPs conjugates is relatively small but statistically significant (p < 0.05), with an average increase of 0.002 RIU (Figure 2h). Overall, these results demonstrate that the attachment of Au NPs is important for producing measurable and significant changes in the external RI upon DNA binding to microlasers.

WGM modes decay exponentially away from the surface of the microlasers or resonators; (44) for the resonator geometry described here, the 1/e extension for a typical TE mode is approximately 120 nm. (18) The observed increase in the average external refractive index is influenced by the full extension, with the highest sensitivity occurring near the surface, where the field overlap is strongest.

Thus, the refractive index measurement does not represent the intrinsic refractive index of DNA or Au NPs alone but rather their combined effect with the buffer medium. When the DNA helix forms, bringing Au NPs closer to the surface, the increased overlap with the evanescent field leads to a higher measured RI.

Next, we examined how the ionic strength and buffer concentration affect the RI measured by microlasers. Microlasers modified with ssDNA-Au NPs were hybridized with complementary csDNA in buffers of varying concentrations. Since the buffer concentration correlates with ionic strength, this approach enabled us to systematically investigate the role of ion shielding on DNA hybridization and compaction. The increased ionic strength corresponds to higher cation concentrations, which effectively shield the negatively charged phosphate groups along the DNA backbone and thus lead to a more stable structure. (45−47) Salt ions weaken the electrostatic repulsion of the phosphates and allow the DNA strands to approach one another, promoting a more compact structure. (48,49)

Figure 3 presents the RI distributions for N > 40 microlasers under different buffer conditions. Figure 3a shows ssDNA-Au NP-functionalized microlasers and provides a baseline for sample-to-sample variations. Upon hybridization with csDNA, a notable upshift in the RI distribution is observed, as shown in Figure 3b for a buffer concentration of 0.01 M. We attribute the increase in RI to the hybridization bringing Au NPs closer to the microlaser surface due to formation of the compact B-form double helix of the DNA. (50)

Figure 3

Figure 3. Detection of DNA compaction at varying ionic strengths of buffer solutions. Histograms of the refractive index of (a) ssDNA-Au NP-functionalized microlasers in a 0.01 M buffer solution (N = 48) and microlasers following hybridization with csDNA in (b) 0.01 M (N = 47) and (c) 0.1 M (N = 49) buffer solutions.

At a higher buffer concentration of 0.1 M, we observed a further increase in RI, with an average change of 0.004 RIU relative to the 0.01 M buffer concentration (p < 0.05). This finding further confirms that an increase in ionic strength increases the compactness of the dsDNA helix, facilitates the closer proximity of the Au NPs to the microlaser surface, and thereby amplifies the RI perceived by the lasing modes.

Having demonstrated that microlasers functionalized with Au NPs provide an effective platform for sensing DNA hybridization and distinguishing different ionic strengths in ensembles of microlasers, we now explore the detection of DNA hybridization of strands with varying lengths. To do so, we follow the RI change in the vicinity of individual microlasers due to hybridization events in real time. Specifically, a microlaser decorated with ssDNA conjugated to a NP at its 5′-terminus is continuously monitored for spectral changes, while csDNA is added in solution (Figure 4a). In Figure 4b, we show a TE/TM pair of WGM modes and follow their shift over the course of the experiment. The corresponding changes in RI, calculated from the spectral shifts, are plotted in Figure 4c. (Additional lasing modes are present in the spectrum but are not displayed for the sake of simplicity.)

Figure 4

Figure 4. Real-time detection of DNA hybridization on the surface of a microlaser. (a) Schematic representation of DNA hybridization on single-stranded DNA (ssDNA) functionalized with Au nanoparticles (Au NPs). (b) Spectral shifts of a selected TM and TE mode from a single microlaser at different time points during the reaction. (c) Transient refractive index change calculated from the microlaser spectra acquired during DNA hybridization on the laser surface. Time zero (t = 0) indicates the moment csDNA was introduced into the solution. Filled diamonds indicate specific time points with corresponding spectra shown in panel b.

Before the addition of csDNA, the spectra and the calculated corresponding RIs remain unchanged, as indicated by the blue and lilac points and spectra in panels c and b, respectively, of Figure 4. Upon introduction of csDNA at time zero, a red-shift in both the TM and TE modes is observed, corresponding to an increase in the RI. Once the system reaches equilibrium, the spectra stabilize, as represented by the green and pink points and spectra in panels c and b, respectively, of Figure 4. As these experiments are not influenced by inherent variability between microlasers (e.g., in size, internal RI, coverage, etc.), they can monitor the binding of molecules in real time and provide drastically improved sensitivity. As such, it is also possible to measure the hybridization of DNA in the absence of Au NPs (Figure S4). To further validate our findings, we also perform measurements on a control sample consisting of carboxylated microlasers without ssDNA attached to the surface. Upon addition of csDNA, no significant increase in the refractive index is observed (Figure S5), confirming that the observed RI shift in our primary experiments is specifically due to DNA hybridization rather than nonspecific interactions.

We also explored different hybridization configurations. The Au NPs were on the ssDNA, csDNA, both, or neither; real-time hybridization curves were obtained, and the changes in refractive index are compared in Figure S6. Notably, the RI change was found to be most pronounced when the Au NPs were attached to the ssDNA, which is the primary focus of this study.

Finally, we developed an inverted microlaser-based test system for DNA sensing, which may also be employed in the future as target-sensitive hairpin-based drug delivery system. (51) To explore this, we employed a six-nucleotide hairpin (HP) sequence construct forming a four-nucleotide loop (51) and modified with Au NPs by amide coupling of COOH-modified Au NPs with amino linker-functionalized hairpin DNA strands on the 5′-end, as detailed in the Methods of the Supporting Information. The baseline RI distribution for microlasers conjugated with a ssDNA (Figure 5a) agrees with the RI values previously seen in samples with ssDNA-NPs (Figure 2g) and hybridized systems containing csDNA (Figure 2h). When adding csDNA, we expected that csDNA replaces the HP, resulting in a decrease in RI by removal of the Au NPs. However, contrary to this expectation, an increase in RI was observed. Binding energy predictions (see Figure S7) and melting temperature measurements (see Figures S8 and S9) indicate that at room temperature (RT), the high binding energies, derived from two sets of three matching base pairs, maintain the stability of the test system. This causes a contraction in the overall construct length, bringing Au NPs closer to the microlaser surface, as observed when the csDNA binds, and consequently increasing the measured RI.

Figure 5

Figure 5. Refractive index change upon addition and substitution of hairpin DNA. (a) Refractive index histogram for microlasers functionalized with ssDNA. (b) Refractive index histogram after addition of the HP33 hairpin. (c–e) Refractive index histograms after substitution was performed by addition of csDNA for a 1 h reaction at (c) room temperature (RT), (d) 37 °C, and (e) 60 °C. Refractive index measurements were performed at RT in all cases.

After performing hybridization at increased temperatures of 37 and 60 °C for 1 h, we observed the anticipated substitution of HP-Au NPs, evidenced by the decrease in the local RI. At 37 °C (Figure 5d), partial removal of HP-Au NPs was observed, with the RI remaining significantly above that of ssDNA-conjugated microlasers. At 60 °C (Figure 5e), nearly complete removal was achieved, and the RI returned to the range observed for unmodified samples (Figure 5a).

In summary, we demonstrated an innovative approach to nucleic acid sensing using WGM microlasers functionalized with DNA and Au NPs. Our method leverages real-time monitoring of RI changes near the microlaser surface, providing a sensitive platform for detecting DNA hybridization and structural dynamics. It enables detection of sequences in two distinct configurations: either by immobilizing the target complementary strand on the laser surface with a Au NP attached to its 5′-end or by binding a bare strand to the laser surface and complementing this with a Au NP-modified hairpin strand. In both scenarios, we successfully detected an unmodified target DNA sequence. Compared to many fluorescence-based methods, our technique requires only minor 5′-end modifications on the DNA, effectively circumventing the issue of fluorophore quenching. (52) The addition of Au NPs significantly enhances the sensitivity of this WGM-based detection as RI changes become more pronounced with nanoparticle proximity. Additionally, we explored the influence of ionic strength on hybridization, showing that variations in ion concentration affect DNA compactness and, consequently, RI shifts. Furthermore, a hairpin-based test system has been developed to assess DNA hybridization as a potential controlled release mechanism, enabling potential applications in targeted drug delivery.

Our findings pave the way for broader applications of WGM microlaser sensors, particularly in areas requiring precise detection of nucleic acid interactions, such as diagnostics and environmental monitoring. This platform enables the use of customizeable DNA sequences tailored to bind various targets, e.g., nucleic acid sequences by base pairing, to small molecules or peptide/proteins using aptamer sequences.

Finally, our platform provides a highly adaptable basis for sequence-specific detection systems. Understanding conformational changes in nucleic acids and investigating biomechanical forces within cells are increasingly important for elucidating cellular functions and molecular interactions. The structural transitions in DNA and RNA─such as folding, hybridization, and denaturation─are critical for processes such as transcription, replication, and signaling. Integration of this system with different capture strands has the potential to enhance multiplexed sensing capabilities, enabling simultaneous monitoring of multiple analytes in complex biological samples, potentially redefining current approaches to nucleic acid detection and analysis.

Data Availability

Click to copy section linkSection link copied!

The research data underpinning this publication can be accessed at https://doi.org/10.15125/BATH-01497. (53)

Supporting Information

Click to copy section linkSection link copied!

The Supporting Information is available free of charge at https://pubs.acs.org/doi/10.1021/acs.nanolett.5c00078.

  • Detailed experimental information (PDF)

Terms & Conditions

Most electronic Supporting Information files are available without a subscription to ACS Web Editions. Such files may be downloaded by article for research use (if there is a public use license linked to the relevant article, that license may permit other uses). Permission may be obtained from ACS for other uses through requests via the RightsLink permission system: http://pubs.acs.org/page/copyright/permissions.html.

Author Information

Click to copy section linkSection link copied!

  • Corresponding Authors
    • Soraya Caixeiro - Department of Chemistry and Biochemistry, Humboldt Centre for Nano- and Biophotonics, Institute for Light and Matter, Greinstrasse 4-6, 50939 Cologne, GermanyCentre for Photonics and Photonic Materials, Department of Physics, University of Bath, Bath BA2 7AY, United KingdomOrcidhttps://orcid.org/0000-0003-4605-957X Email: [email protected]
    • Stephanie Kath-Schorr - Department of Chemistry and Biochemistry, Institute of Organic Chemistry, Greinstrasse 4, 50939 Cologne, GermanyOrcidhttps://orcid.org/0000-0002-5180-360X Email: [email protected]
    • Malte C. Gather - Department of Chemistry and Biochemistry, Humboldt Centre for Nano- and Biophotonics, Institute for Light and Matter, Greinstrasse 4-6, 50939 Cologne, GermanyCentre of Biophotonics, SUPA School of Physics and Astronomy, University of St Andrews, St Andrews KY16 9SS, United KingdomOrcidhttps://orcid.org/0000-0002-4857-5562 Email: [email protected]
  • Authors
    • Robert Dörrenhaus - Department of Chemistry and Biochemistry, Institute of Organic Chemistry, Greinstrasse 4, 50939 Cologne, GermanyOrcidhttps://orcid.org/0009-0006-4685-9939
    • Anna Popczyk - Department of Chemistry and Biochemistry, Humboldt Centre for Nano- and Biophotonics, Institute for Light and Matter, Greinstrasse 4-6, 50939 Cologne, Germany
    • Marcel Schubert - Department of Chemistry and Biochemistry, Humboldt Centre for Nano- and Biophotonics, Institute for Light and Matter, Greinstrasse 4-6, 50939 Cologne, Germany
  • Author Contributions

    S.C. and R.D. contributed equally to this work.

  • Funding

    This work received financial support from the Humboldt Foundation (Alexander von Humboldt professorship to M.C.G.).

  • Notes
    The authors declare no competing financial interest.

    The research data underpinning this publication can be accessed at https://doi.org/10.15125/BATH-01497 (ref 53).

Acknowledgments

Click to copy section linkSection link copied!

The authors thank Prof. Jan Riemer for fruitful discussions.

References

Click to copy section linkSection link copied!

This article references 53 other publications.

  1. 1
    Lächelt, U.; Wagner, E. Nucleic Acid Therapeutics Using Polyplexes: A Journey of 50 Years (and Beyond). Chem. Rev. 2015, 115, 1104311078,  DOI: 10.1021/cr5006793
  2. 2
    Benner, S. A. Understanding nucleic acids using synthetic chemistry. Acc. Chem. Res. 2004, 37, 784797,  DOI: 10.1021/ar040004z
  3. 3
    Minchin, S.; Lodge, J. Understanding biochemistry: Structure and function of nucleic acids. Essays Biochem 2019, 63, 433456,  DOI: 10.1042/EBC20180038
  4. 4
    Travers, A.; Muskhelishvili, G. DNA structure and function. FEBS J. 2015, 282, 22792295,  DOI: 10.1111/febs.13307
  5. 5
    Schroeder, R.; Barta, A.; Semrad, K. Strategies for RNA folding and assembly. Nat. Rev. Mol. Cell Biol. 2004, 5, 908919,  DOI: 10.1038/nrm1497
  6. 6
    Saccà, B.; Niemeyer, C. M. DNA origami: The art of folding DNA. Angew. Chemie - Int. Ed. 2012, 51, 5866,  DOI: 10.1002/anie.201105846
  7. 7
    Fallmann, J. Recent advances in RNA folding. J. Biotechnol. 2017, 261, 97104,  DOI: 10.1016/j.jbiotec.2017.07.007
  8. 8
    Fakih, H. H.; Itani, M. M.; Karam, P. Gold nanoparticles-coated polystyrene beads for the multiplex detection of viral DNA. Sensors Actuators, B Chem. 2017, 250, 446452,  DOI: 10.1016/j.snb.2017.04.066
  9. 9
    Qi, Y.; Song, D.; Chen, Y. Colorimetric oligonucleotide-based sensor for ultra-low Hg2+ in contaminated environmental medium: Convenience, sensitivity and mechanism. Sci. Total Environ. 2021, 766, 142579,  DOI: 10.1016/j.scitotenv.2020.142579
  10. 10
    García-Mendiola, T. Functionalization of a Few-Layer Antimonene with Oligonucleotides for DNA Sensing. ACS Appl. Nano Mater. 2020, 3, 36253633,  DOI: 10.1021/acsanm.0c00335
  11. 11
    Ambartsumyan, O.; Gribanyov, D.; Kukushkin, V.; Kopylov, A.; Zavyalova, E. SERS-based biosensors for virus determination with oligonucleotides as recognition elements. Int. J. Mol. Sci. 2020, 21, 3373,  DOI: 10.3390/ijms21093373
  12. 12
    Zheng, J.; Chen, C.; Wang, X.; Zhang, F.; He, P. A sequence-specific DNA sensor for Hepatitis B virus diagnostics based on the host-guest recognition. Sensors Actuators, B Chem. 2014, 199, 168174,  DOI: 10.1016/j.snb.2014.03.110
  13. 13
    Paludan, S. R.; Bowie, A. G. Immune Sensing of DNA. Immunity 2013, 38, 870880,  DOI: 10.1016/j.immuni.2013.05.004
  14. 14
    Huang, K. J. Signal amplification for electrochemical DNA biosensor based on two-dimensional graphene analogue tungsten sulfide-graphene composites and gold nanoparticles. Sensors Actuators, B Chem. 2014, 191, 828836,  DOI: 10.1016/j.snb.2013.10.072
  15. 15
    Toropov, N. Review of biosensing with whispering-gallery mode lasers. Light: Sci. Appl. 2021, 10, 42,  DOI: 10.1038/s41377-021-00471-3
  16. 16
    Fan, X.; Yun, S.-H. The potential of optofluidic biolasers. Nat. Methods 2014, 11, 1417,  DOI: 10.1038/nmeth.2805
  17. 17
    Pan, T.; Lu, D.; Xin, H.; Li, B. Biophotonic probes for bio-detection and imaging. Light: Sci. Appl. 2021, 10, 124,  DOI: 10.1038/s41377-021-00561-2
  18. 18
    Caixeiro, S. Local Sensing of Absolute Refractive Index During Protein-Binding using Microlasers with Spectral Encoding. Adv. Opt. Mater. 2023, 11, 2300530,  DOI: 10.1002/adom.202300530
  19. 19
    Schubert, M. Monitoring contractility in cardiac tissue with cellular resolution using biointegrated microlasers. Nat. Photonics 2020, 14, 452458,  DOI: 10.1038/s41566-020-0631-z
  20. 20
    Caixeiro, S.; Gaio, M.; Marelli, B.; Omenetto, F. G.; Sapienza, R. Silk-Based Biocompatible Random Lasing. Adv. Opt. Mater. 2016, 4, 9981003,  DOI: 10.1002/adom.201600185
  21. 21
    Wang, Y. Demonstration of intracellular real-time molecular quantification via FRET-enhanced optical microcavity. Nat. Commun. 2022, 13, 6685,  DOI: 10.1038/s41467-022-34547-4
  22. 22
    Duan, R.; Hao, X.; Li, Y.; Li, H. Detection of acetylcholinesterase and its inhibitors by liquid crystal biosensor based on whispering gallery mode. Sensors Actuators, B Chem. 2020, 308, 127672,  DOI: 10.1016/j.snb.2020.127672
  23. 23
    Schubert, M. Lasing within Live Cells Containing Intracellular Optical Microresonators for Barcode-Type Cell Tagging and Tracking. Nano Lett. 2015, 15, 56475652,  DOI: 10.1021/acs.nanolett.5b02491
  24. 24
    Martino, N. Wavelength-encoded laser particles for massively multiplexed cell tagging. Nat. Photonics 2019, 13, 720727,  DOI: 10.1038/s41566-019-0489-0
  25. 25
    Fikouras, A. H. Non-obstructive intracellular nanolasers. Nat. Commun. 2018, 9, 4817,  DOI: 10.1038/s41467-018-07248-0
  26. 26
    Dalaka, E. Deformable microlaser force sensing. Light: Sci. Appl. 2024, 13, 129,  DOI: 10.1038/s41377-024-01471-9
  27. 27
    Pirnat, G.; Marinčič, M.; Ravnik, M.; Humar, M. Quantifying local stiffness and forces in soft biological tissues using droplet optical microcavities. Proc. Natl. Acad. Sci. U. S. A. 2024, 121 (4), e2314884121  DOI: 10.1073/pnas.2314884121
  28. 28
    Leonetti, M. Optical gain in DNA-DCM for lasing in photonic materials. Opt. Lett. 2009, 34, 37643766,  DOI: 10.1364/OL.34.003764
  29. 29
    Lee, W.; Chen, Q.; Fan, X.; Yoon, D. K. Digital DNA detection based on a compact optofluidic laser with ultra-low sample consumption. Lab Chip 2016, 16, 47704776,  DOI: 10.1039/C6LC01258B
  30. 30
    Tanwar, S.; Kaur, V.; Kaur, G.; Sen, T. Broadband SERS Enhancement by DNA Origami Assembled Bimetallic Nanoantennas with Label-Free Single Protein Sensing. J. Phys. Chem. Lett. 2021, 12, 81418150,  DOI: 10.1021/acs.jpclett.1c02272
  31. 31
    Das, M.; Shim, K. H.; An, S. S. A.; Yi, D. K. Review on gold nanoparticles and their applications. Toxicol. Environ. Health Sci. 2011, 3, 193205,  DOI: 10.1007/s13530-011-0109-y
  32. 32
    Dreaden, E. C.; Alkilany, A. M.; Huang, X.; Murphy, C. J.; El-Sayed, M. A. The golden age: Gold nanoparticles for biomedicine. Chem. Soc. Rev. 2012, 41, 27402779,  DOI: 10.1039/C1CS15237H
  33. 33
    Hao, Y.; Fang, L.; Deng, Z. Solvo-driven dimeric nanoplasmon coupling under DNA direction. CCS Chem. 2021, 3, 13591367,  DOI: 10.31635/ccschem.020.202000290
  34. 34
    Wang, P. Magnetic Plasmon Networks Programmed by Molecular Self-Assembly. Adv. Mater. 2019, 31, 1901364,  DOI: 10.1002/adma.201901364
  35. 35
    Xie, M.; Jiang, J.; Chao, J. DNA-Based Gold Nanoparticle Assemblies: From Structure Constructions to Sensing Applications. Sensors 2023, 23, 9229,  DOI: 10.3390/s23229229
  36. 36
    Park, D. J. Directional emission from dye-functionalized plasmonic DNA superlattice microcavities. Proc. Natl. Acad. Sci. U. S. A. 2017, 114, 457461,  DOI: 10.1073/pnas.1619802114
  37. 37
    Wu, F. C.; Wu, Y.; Niu, Z.; Vollmer, F. Ratiometric detection of oligonucleotide stoichiometry on multi-functional gold nanoparticles by whispering gallery mode biosensing. Analyst 2015, 140, 29692972,  DOI: 10.1039/C5AN00179J
  38. 38
    Li, L.; Zhang, Y.-n.; Zheng, W.; Li, X.; Zhao, Y. Optical fiber SPR biosensor based on gold nanoparti-cle amplification for DNA hybridization detection. Talanta 2022, 247, 123599,  DOI: 10.1016/j.talanta.2022.123599
  39. 39
    Baaske, M. D.; Foreman, M. R.; Vollmer, F. Single-molecule nucleic acid interactions monitored on a label-free microcavity biosensor platform. Nat. Nanotechnol. 2014, 9, 933939,  DOI: 10.1038/nnano.2014.180
  40. 40
    de Planell-Saguer, M.; Rodicio, M. C.; Mourelatos, Z. Rapid in situ codetection of noncoding RNAs and proteins in cells and formalin-fixed paraffin-embedded tissue sections without protease treatment. Nat. Protoc. 2010, 5, 10611073,  DOI: 10.1038/nprot.2010.62
  41. 41
    Nuovo, G. J.; Lee, E. J.; Lawler, S.; Godlewski, J.; Schmittgen, T. D. In situ detection of mature microRNAs by labeled extension on ultramer templates. Biotechniques 2009, 46, 115126,  DOI: 10.2144/000113068
  42. 42
    Pena, J. T. G. miRNA in situ hybridization in formaldehyde and EDC - Fixed tissues. Nat. Methods 2009, 6, 139141,  DOI: 10.1038/nmeth.1294
  43. 43
    Titze, V. M. Hyperspectral confocal imaging for high-throughput readout and analysis of bio-integrated microlasers. Nat. Protoc. 2024, 19, 928959,  DOI: 10.1038/s41596-023-00924-6
  44. 44
    Foreman, M. R.; Swaim, J. D.; Vollmer, F. Whispering gallery mode sensors. Adv. Opt. Photonics 2015, 7, 168240,  DOI: 10.1364/AOP.7.000168
  45. 45
    Owczarzy, R.; Moreira, B. G.; You, Y.; Behlke, M. A.; Wälder, J. A. Predicting stability of DNA duplexes in solutions containing magnesium and monovalent cations. Biochemistry 2008, 47, 53365353,  DOI: 10.1021/bi702363u
  46. 46
    Morris, D. L. DNA-bound metal ions: Recent developments. Biomol. Concepts 2014, 5, 397407,  DOI: 10.1515/bmc-2014-0021
  47. 47
    Wetmur, J. G.; Fresco, J. DNA probes: Applications of the principles of nucleic acid hybridization. Crit. Rev. Biochem. Mol. Biol. 1991, 26, 227259,  DOI: 10.3109/10409239109114069
  48. 48
    Draper, D. E. Folding of RNA tertiary structure: Linkages between backbone phosphates, ions, and water. Biopolymers 2013, 99, 11051113,  DOI: 10.1002/bip.22249
  49. 49
    Tan, Z. J.; Chen, S. J. Nucleic acid helix stability: Effects of salt concentration, cation valence and size, and chain length. Biophys. J. 2006, 90, 11751190,  DOI: 10.1529/biophysj.105.070904
  50. 50
    Wang, G.; Vasquez, K. M. Impact of alternative DNA structures on DNA damage, DNA repair, and genetic instability. DNA Repair (Amst). 2014, 19, 143151,  DOI: 10.1016/j.dnarep.2014.03.017
  51. 51
    Shan, L. Hairpin DNA-Based Nanomaterials for Tumor Targeting and Synergistic Therapy. Int. J. Nanomedicine 2024, 19, 57815792,  DOI: 10.2147/IJN.S461774
  52. 52
    Epstein, J. R.; Biran, I.; Walt, D. R. Fluorescence-Based Nucleic Acid Detection and Microarrays ; 2002; Vol. 469.
  53. 53
    Caixeiro, S., Dörrenhaus, R., Popczyk, A., Schubert, M., Kath-Schorr, S., Gather, M. C., in press. Dataset for “DNA Sensing with Whispering Gallery Mode Microlaser”. Bath: University of Bath Research Data Archive.  DOI: 10.15125/BATH-01497 .

Cited By

Click to copy section linkSection link copied!
Citation Statements
Explore this article's citation statements on scite.ai

This article is cited by 1 publications.

  1. Evgeniia O. Soloveva, Natalia N. Shevchenko, Nikita S. Kirilkin, Albert A. Rogachev, Mariia S. Kovova, Alexander S. Timin, Vladislava A. Rusakova, Sergei A. Shipilovskikh, Anton A. Starovoytov, Daler R. Dadadzhanov, Nikita Toropov. Inherent luminescence in undoped polystyrene microbeads supporting whispering-gallery modes. Optical Materials 2025, 165 , 117058. https://doi.org/10.1016/j.optmat.2025.117058

Nano Letters

Cite this: Nano Lett. 2025, 25, 11, 4467–4475
Click to copy citationCitation copied!
https://doi.org/10.1021/acs.nanolett.5c00078
Published March 4, 2025

Copyright © 2025 The Authors. Published by American Chemical Society. This publication is licensed under

CC-BY 4.0 .

Article Views

1100

Altmetric

-

Citations

Learn about these metrics

Article Views are the COUNTER-compliant sum of full text article downloads since November 2008 (both PDF and HTML) across all institutions and individuals. These metrics are regularly updated to reflect usage leading up to the last few days.

Citations are the number of other articles citing this article, calculated by Crossref and updated daily. Find more information about Crossref citation counts.

The Altmetric Attention Score is a quantitative measure of the attention that a research article has received online. Clicking on the donut icon will load a page at altmetric.com with additional details about the score and the social media presence for the given article. Find more information on the Altmetric Attention Score and how the score is calculated.

  • Abstract

    Figure 1

    Figure 1. Preparation and optical characterization of the surface coating with gold nanoparticle (Au NP)-functionalized DNA on microlasers. (a) Schematic of the nanoparticle ssDNA conjugation to a carboxyl-functionalized microlaser. (b) Electron microscopy image of a carboxyl-functionalized microlaser. The scale bar is 2 μm. (c) Electron microscopy image of a microlaser decorated with DNA functionalized with 40 nm diameter Au NPs. Scale bars are 2 μm and 500 nm (inset). (e) Green fluorescence from a microlaser functionalized with ssDNA with Cy5 dye. (f) Red fluorescence of same microlaser. (g) Overlay of green and red emission. (h–j) Microlaser with dye-free ssDNA on the surface showing no red fluorescence (h). The hybridization with csDNA containing Cy5 illustrated in panel i leads to the appearance of a red ring in the fluorescence image (j). Scale bars for panels e–h and j are 20 μm.

    Figure 2

    Figure 2. Refractive index sensing of DNA surface modifications. (a) Representative lasing spectra from a microlaser in a buffered solution, along with the fitted refractive index. (b) Simulated lasing spectra for microlasers embedded in media of two different refractive indices: n = 1.340 (orange), and n = 1.345 (blue). (c) Close-up of the simulated spectra, highlighting the spectral shifts across different refractive indices and polarization, for azimuthal mode number m = 105. Histograms of external refractive indices calculated from measured laser spectra, with a corresponding box plot, showing (d) carboxyl-functionalized microlasers (N = 71), (e) microlasers conjugated with ssDNA (N = 99), (f) microlasers conjugated with dsDNA (N = 90), (g) microlasers conjugated with ssDNA and Au NPs (N = 65), and (h) microlasers conjugated with dsDNA and Au NPs (N = 91). The illustrations to the right of each histogram depict the configuration for each case.

    Figure 3

    Figure 3. Detection of DNA compaction at varying ionic strengths of buffer solutions. Histograms of the refractive index of (a) ssDNA-Au NP-functionalized microlasers in a 0.01 M buffer solution (N = 48) and microlasers following hybridization with csDNA in (b) 0.01 M (N = 47) and (c) 0.1 M (N = 49) buffer solutions.

    Figure 4

    Figure 4. Real-time detection of DNA hybridization on the surface of a microlaser. (a) Schematic representation of DNA hybridization on single-stranded DNA (ssDNA) functionalized with Au nanoparticles (Au NPs). (b) Spectral shifts of a selected TM and TE mode from a single microlaser at different time points during the reaction. (c) Transient refractive index change calculated from the microlaser spectra acquired during DNA hybridization on the laser surface. Time zero (t = 0) indicates the moment csDNA was introduced into the solution. Filled diamonds indicate specific time points with corresponding spectra shown in panel b.

    Figure 5

    Figure 5. Refractive index change upon addition and substitution of hairpin DNA. (a) Refractive index histogram for microlasers functionalized with ssDNA. (b) Refractive index histogram after addition of the HP33 hairpin. (c–e) Refractive index histograms after substitution was performed by addition of csDNA for a 1 h reaction at (c) room temperature (RT), (d) 37 °C, and (e) 60 °C. Refractive index measurements were performed at RT in all cases.

  • References


    This article references 53 other publications.

    1. 1
      Lächelt, U.; Wagner, E. Nucleic Acid Therapeutics Using Polyplexes: A Journey of 50 Years (and Beyond). Chem. Rev. 2015, 115, 1104311078,  DOI: 10.1021/cr5006793
    2. 2
      Benner, S. A. Understanding nucleic acids using synthetic chemistry. Acc. Chem. Res. 2004, 37, 784797,  DOI: 10.1021/ar040004z
    3. 3
      Minchin, S.; Lodge, J. Understanding biochemistry: Structure and function of nucleic acids. Essays Biochem 2019, 63, 433456,  DOI: 10.1042/EBC20180038
    4. 4
      Travers, A.; Muskhelishvili, G. DNA structure and function. FEBS J. 2015, 282, 22792295,  DOI: 10.1111/febs.13307
    5. 5
      Schroeder, R.; Barta, A.; Semrad, K. Strategies for RNA folding and assembly. Nat. Rev. Mol. Cell Biol. 2004, 5, 908919,  DOI: 10.1038/nrm1497
    6. 6
      Saccà, B.; Niemeyer, C. M. DNA origami: The art of folding DNA. Angew. Chemie - Int. Ed. 2012, 51, 5866,  DOI: 10.1002/anie.201105846
    7. 7
      Fallmann, J. Recent advances in RNA folding. J. Biotechnol. 2017, 261, 97104,  DOI: 10.1016/j.jbiotec.2017.07.007
    8. 8
      Fakih, H. H.; Itani, M. M.; Karam, P. Gold nanoparticles-coated polystyrene beads for the multiplex detection of viral DNA. Sensors Actuators, B Chem. 2017, 250, 446452,  DOI: 10.1016/j.snb.2017.04.066
    9. 9
      Qi, Y.; Song, D.; Chen, Y. Colorimetric oligonucleotide-based sensor for ultra-low Hg2+ in contaminated environmental medium: Convenience, sensitivity and mechanism. Sci. Total Environ. 2021, 766, 142579,  DOI: 10.1016/j.scitotenv.2020.142579
    10. 10
      García-Mendiola, T. Functionalization of a Few-Layer Antimonene with Oligonucleotides for DNA Sensing. ACS Appl. Nano Mater. 2020, 3, 36253633,  DOI: 10.1021/acsanm.0c00335
    11. 11
      Ambartsumyan, O.; Gribanyov, D.; Kukushkin, V.; Kopylov, A.; Zavyalova, E. SERS-based biosensors for virus determination with oligonucleotides as recognition elements. Int. J. Mol. Sci. 2020, 21, 3373,  DOI: 10.3390/ijms21093373
    12. 12
      Zheng, J.; Chen, C.; Wang, X.; Zhang, F.; He, P. A sequence-specific DNA sensor for Hepatitis B virus diagnostics based on the host-guest recognition. Sensors Actuators, B Chem. 2014, 199, 168174,  DOI: 10.1016/j.snb.2014.03.110
    13. 13
      Paludan, S. R.; Bowie, A. G. Immune Sensing of DNA. Immunity 2013, 38, 870880,  DOI: 10.1016/j.immuni.2013.05.004
    14. 14
      Huang, K. J. Signal amplification for electrochemical DNA biosensor based on two-dimensional graphene analogue tungsten sulfide-graphene composites and gold nanoparticles. Sensors Actuators, B Chem. 2014, 191, 828836,  DOI: 10.1016/j.snb.2013.10.072
    15. 15
      Toropov, N. Review of biosensing with whispering-gallery mode lasers. Light: Sci. Appl. 2021, 10, 42,  DOI: 10.1038/s41377-021-00471-3
    16. 16
      Fan, X.; Yun, S.-H. The potential of optofluidic biolasers. Nat. Methods 2014, 11, 1417,  DOI: 10.1038/nmeth.2805
    17. 17
      Pan, T.; Lu, D.; Xin, H.; Li, B. Biophotonic probes for bio-detection and imaging. Light: Sci. Appl. 2021, 10, 124,  DOI: 10.1038/s41377-021-00561-2
    18. 18
      Caixeiro, S. Local Sensing of Absolute Refractive Index During Protein-Binding using Microlasers with Spectral Encoding. Adv. Opt. Mater. 2023, 11, 2300530,  DOI: 10.1002/adom.202300530
    19. 19
      Schubert, M. Monitoring contractility in cardiac tissue with cellular resolution using biointegrated microlasers. Nat. Photonics 2020, 14, 452458,  DOI: 10.1038/s41566-020-0631-z
    20. 20
      Caixeiro, S.; Gaio, M.; Marelli, B.; Omenetto, F. G.; Sapienza, R. Silk-Based Biocompatible Random Lasing. Adv. Opt. Mater. 2016, 4, 9981003,  DOI: 10.1002/adom.201600185
    21. 21
      Wang, Y. Demonstration of intracellular real-time molecular quantification via FRET-enhanced optical microcavity. Nat. Commun. 2022, 13, 6685,  DOI: 10.1038/s41467-022-34547-4
    22. 22
      Duan, R.; Hao, X.; Li, Y.; Li, H. Detection of acetylcholinesterase and its inhibitors by liquid crystal biosensor based on whispering gallery mode. Sensors Actuators, B Chem. 2020, 308, 127672,  DOI: 10.1016/j.snb.2020.127672
    23. 23
      Schubert, M. Lasing within Live Cells Containing Intracellular Optical Microresonators for Barcode-Type Cell Tagging and Tracking. Nano Lett. 2015, 15, 56475652,  DOI: 10.1021/acs.nanolett.5b02491
    24. 24
      Martino, N. Wavelength-encoded laser particles for massively multiplexed cell tagging. Nat. Photonics 2019, 13, 720727,  DOI: 10.1038/s41566-019-0489-0
    25. 25
      Fikouras, A. H. Non-obstructive intracellular nanolasers. Nat. Commun. 2018, 9, 4817,  DOI: 10.1038/s41467-018-07248-0
    26. 26
      Dalaka, E. Deformable microlaser force sensing. Light: Sci. Appl. 2024, 13, 129,  DOI: 10.1038/s41377-024-01471-9
    27. 27
      Pirnat, G.; Marinčič, M.; Ravnik, M.; Humar, M. Quantifying local stiffness and forces in soft biological tissues using droplet optical microcavities. Proc. Natl. Acad. Sci. U. S. A. 2024, 121 (4), e2314884121  DOI: 10.1073/pnas.2314884121
    28. 28
      Leonetti, M. Optical gain in DNA-DCM for lasing in photonic materials. Opt. Lett. 2009, 34, 37643766,  DOI: 10.1364/OL.34.003764
    29. 29
      Lee, W.; Chen, Q.; Fan, X.; Yoon, D. K. Digital DNA detection based on a compact optofluidic laser with ultra-low sample consumption. Lab Chip 2016, 16, 47704776,  DOI: 10.1039/C6LC01258B
    30. 30
      Tanwar, S.; Kaur, V.; Kaur, G.; Sen, T. Broadband SERS Enhancement by DNA Origami Assembled Bimetallic Nanoantennas with Label-Free Single Protein Sensing. J. Phys. Chem. Lett. 2021, 12, 81418150,  DOI: 10.1021/acs.jpclett.1c02272
    31. 31
      Das, M.; Shim, K. H.; An, S. S. A.; Yi, D. K. Review on gold nanoparticles and their applications. Toxicol. Environ. Health Sci. 2011, 3, 193205,  DOI: 10.1007/s13530-011-0109-y
    32. 32
      Dreaden, E. C.; Alkilany, A. M.; Huang, X.; Murphy, C. J.; El-Sayed, M. A. The golden age: Gold nanoparticles for biomedicine. Chem. Soc. Rev. 2012, 41, 27402779,  DOI: 10.1039/C1CS15237H
    33. 33
      Hao, Y.; Fang, L.; Deng, Z. Solvo-driven dimeric nanoplasmon coupling under DNA direction. CCS Chem. 2021, 3, 13591367,  DOI: 10.31635/ccschem.020.202000290
    34. 34
      Wang, P. Magnetic Plasmon Networks Programmed by Molecular Self-Assembly. Adv. Mater. 2019, 31, 1901364,  DOI: 10.1002/adma.201901364
    35. 35
      Xie, M.; Jiang, J.; Chao, J. DNA-Based Gold Nanoparticle Assemblies: From Structure Constructions to Sensing Applications. Sensors 2023, 23, 9229,  DOI: 10.3390/s23229229
    36. 36
      Park, D. J. Directional emission from dye-functionalized plasmonic DNA superlattice microcavities. Proc. Natl. Acad. Sci. U. S. A. 2017, 114, 457461,  DOI: 10.1073/pnas.1619802114
    37. 37
      Wu, F. C.; Wu, Y.; Niu, Z.; Vollmer, F. Ratiometric detection of oligonucleotide stoichiometry on multi-functional gold nanoparticles by whispering gallery mode biosensing. Analyst 2015, 140, 29692972,  DOI: 10.1039/C5AN00179J
    38. 38
      Li, L.; Zhang, Y.-n.; Zheng, W.; Li, X.; Zhao, Y. Optical fiber SPR biosensor based on gold nanoparti-cle amplification for DNA hybridization detection. Talanta 2022, 247, 123599,  DOI: 10.1016/j.talanta.2022.123599
    39. 39
      Baaske, M. D.; Foreman, M. R.; Vollmer, F. Single-molecule nucleic acid interactions monitored on a label-free microcavity biosensor platform. Nat. Nanotechnol. 2014, 9, 933939,  DOI: 10.1038/nnano.2014.180
    40. 40
      de Planell-Saguer, M.; Rodicio, M. C.; Mourelatos, Z. Rapid in situ codetection of noncoding RNAs and proteins in cells and formalin-fixed paraffin-embedded tissue sections without protease treatment. Nat. Protoc. 2010, 5, 10611073,  DOI: 10.1038/nprot.2010.62
    41. 41
      Nuovo, G. J.; Lee, E. J.; Lawler, S.; Godlewski, J.; Schmittgen, T. D. In situ detection of mature microRNAs by labeled extension on ultramer templates. Biotechniques 2009, 46, 115126,  DOI: 10.2144/000113068
    42. 42
      Pena, J. T. G. miRNA in situ hybridization in formaldehyde and EDC - Fixed tissues. Nat. Methods 2009, 6, 139141,  DOI: 10.1038/nmeth.1294
    43. 43
      Titze, V. M. Hyperspectral confocal imaging for high-throughput readout and analysis of bio-integrated microlasers. Nat. Protoc. 2024, 19, 928959,  DOI: 10.1038/s41596-023-00924-6
    44. 44
      Foreman, M. R.; Swaim, J. D.; Vollmer, F. Whispering gallery mode sensors. Adv. Opt. Photonics 2015, 7, 168240,  DOI: 10.1364/AOP.7.000168
    45. 45
      Owczarzy, R.; Moreira, B. G.; You, Y.; Behlke, M. A.; Wälder, J. A. Predicting stability of DNA duplexes in solutions containing magnesium and monovalent cations. Biochemistry 2008, 47, 53365353,  DOI: 10.1021/bi702363u
    46. 46
      Morris, D. L. DNA-bound metal ions: Recent developments. Biomol. Concepts 2014, 5, 397407,  DOI: 10.1515/bmc-2014-0021
    47. 47
      Wetmur, J. G.; Fresco, J. DNA probes: Applications of the principles of nucleic acid hybridization. Crit. Rev. Biochem. Mol. Biol. 1991, 26, 227259,  DOI: 10.3109/10409239109114069
    48. 48
      Draper, D. E. Folding of RNA tertiary structure: Linkages between backbone phosphates, ions, and water. Biopolymers 2013, 99, 11051113,  DOI: 10.1002/bip.22249
    49. 49
      Tan, Z. J.; Chen, S. J. Nucleic acid helix stability: Effects of salt concentration, cation valence and size, and chain length. Biophys. J. 2006, 90, 11751190,  DOI: 10.1529/biophysj.105.070904
    50. 50
      Wang, G.; Vasquez, K. M. Impact of alternative DNA structures on DNA damage, DNA repair, and genetic instability. DNA Repair (Amst). 2014, 19, 143151,  DOI: 10.1016/j.dnarep.2014.03.017
    51. 51
      Shan, L. Hairpin DNA-Based Nanomaterials for Tumor Targeting and Synergistic Therapy. Int. J. Nanomedicine 2024, 19, 57815792,  DOI: 10.2147/IJN.S461774
    52. 52
      Epstein, J. R.; Biran, I.; Walt, D. R. Fluorescence-Based Nucleic Acid Detection and Microarrays ; 2002; Vol. 469.
    53. 53
      Caixeiro, S., Dörrenhaus, R., Popczyk, A., Schubert, M., Kath-Schorr, S., Gather, M. C., in press. Dataset for “DNA Sensing with Whispering Gallery Mode Microlaser”. Bath: University of Bath Research Data Archive.  DOI: 10.15125/BATH-01497 .
  • Supporting Information

    Supporting Information


    The Supporting Information is available free of charge at https://pubs.acs.org/doi/10.1021/acs.nanolett.5c00078.

    • Detailed experimental information (PDF)


    Terms & Conditions

    Most electronic Supporting Information files are available without a subscription to ACS Web Editions. Such files may be downloaded by article for research use (if there is a public use license linked to the relevant article, that license may permit other uses). Permission may be obtained from ACS for other uses through requests via the RightsLink permission system: http://pubs.acs.org/page/copyright/permissions.html.