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# Circularly polarised luminescence laser scanning confocal microscopy to study live cell chiral molecular interactions

## Abstract

The molecular machinery of life is founded on chiral building blocks, but no experimental technique is currently available to distinguish or monitor chiral systems in live cell bio-imaging studies. Luminescent chiral molecules encode a unique optical fingerprint within emitted circularly polarized light (CPL) carrying information about the molecular environment, conformation, and binding state. Here, we present a CPL Laser Scanning Confocal Microscope (CPL-LSCM) capable of simultaneous chiroptical contrast based live-cell imaging of endogenous and engineered CPL-active cellular probes. Further, we demonstrate that CPL-active probes can be activated using two-photon excitation, with complete CPL spectrum recovery. The combination of these two milestone results empowers the multidisciplinary imaging community, allowing the study of chiral interactions on a sub-cellular level in a new (chiral) light.

## Introduction

Chirality is intrinsic to the fundamentals of life, with chiral molecules playing pivotal roles in natural cell homoeostasis, chemical signalling, enzymatic reactions, gene expression and reproduction1. Selective chiral recognition of vital bio-molecules and bioprocesses by specifically designed probes in biological environments, like live cells, is a topic of great interest from both biochemical and analytical application points of view. Tracking chiral molecules within live cells can be of great importance to understanding interactions between cell organelles and drugs or chiral probes. It has been shown that chirality can have a profound effect on drug activity and on localisation in cells amongst others. Stereoselectivity, particularly enantioselectivity is of crucial importance when designing either drugs and/ or molecular probes to interact with proteins2,3. Despite life being founded on chiral building blocks, currently, there are no direct techniques capable of distinguishing and tracking the behaviour of enantiomers in chiral molecular systems—e.g. luminescent probes or proteins—and their individual interactions within living cells.

Circular polarisation luminescence (CPL) spectroscopy and circular dichroism (CD) spectroscopy are optical spectroscopic tools for studying chiral molecules and their interactions, but to date, these have not met the complex biocompatible requirements needed to study and track chiral interactions within cells. CD spectroscopy quantifies how chiral molecules absorb left and right circularly polarised light differentially. CD microscopes have been developed and applied to applications such as the microscopy of inorganic chiral substrates and structures, but CD microscopes face several limitations, including artefacts associated with the linearly polarised light components and optical distortion4,5,6,7. Fundamentally, CD techniques are limited by the optical absorbance of the sample, rendering CD too insensitive and of little use for live-cell imaging.

On the other hand, CPL spectroscopy enables the study of chiral interactions of luminescent molecular systems. Efficient CPL probe complexes, foremost lanthanide coordination complexes, can be used for cellular imaging because of their demonstrated biocompatibility and unique photophysical and CPL properties8. The chirality of such complexes and their binding motifs enables them to be exploited as sub-cellular chiral probes9. However, CPL spectroscopy and measurement technology has lagged behind the development of CPL-active probes, hindering the translation to sub-cellular CPL microscopy. Since the inception of CPL spectrometers roughly 50 years ago photoelastic modulators (PEMs) have been incorporated for circular polarisation analysis, in combination with scanning monochromators for wavelength specificity. Such setups have resulted in bulky, expensive instruments with slow spectral data acquisition rates (~1 h for a typical CPL spectrum)10,11. Consequently, the few CPL microscopes which have been developed incorporate PEMs, and they, therefore, suffer from inherently slow-acquisition rates which are incompatible with imaging CPL within living cells due to: (a) high-energy excitation (e.g. UV/blue) induced phototoxicity and (b) correspondingly poor spatial resolution owing to increased acquisition times. Consequently, circularly polarised emission microscopy studies have been limited to investigations of inert, bulk samples at the millimetre scale, e.g. large inorganic crystals12, or imaging maps of chiral amino acids distributed within agarose gel13. This situation is in stark contrast to the many advances in optical microscopy over recent decades, which have enabled diffraction-limited and super-resolved cellular imaging14.

To advance CPL microscopy, we have previously built a proof-of-concept chiroptical contrast time-resolved epifluorescence microscope and demonstrated enantioselective differential chiral contrast (EDCC) imaging, examining the Λ- and Δ-enantiomers of a bright CPL-active europium complex (Eu:L1, Eu[1,4,7- tris({4-[2-(4- methoxy-2- methylphenyl)ethynyl]-6-[carboxy(phenyl)phosphoryl]pyridin-2-yl}methyl)-1,4,7- triazacyclononane]) (structure depicted on Fig. 3) absorbed onto an optical brightener-free paper test substrate9. This study showed that the enantiomers could be spatially discriminated by their CPL emission profile. This epifluorescence CPL microscope was considerably faster than PEM-CPL microscopes (2 min vs. 40 min total image acquisition), but still required sequential manual selection of CPL detection channels, which is impractical for sub-cellular imaging where high spatio-temporal resolution is necessary to track chiral interactions without the introduction of image artefacts. A microscope capable of simultaneously measuring left and right-handed CPL (ideally with confocal sectioning and truly diffraction-limited resolution) represents a step-change in technological capability, opening up new opportunities to study chiral molecular interactions.

We recently introduced next-generation CPL spectrometer technology which circumvents the aforementioned hindrances of 20th century CPL spectroscopy technology, using a patented optical layout and rapid charge-coupled device (CCD) spectrometers15.

Here, we demonstrate the extension of this rapid CPL measurement technology to CPL laser scanning confocal microscopy (CPL-LSCM). This approach allows the simultaneous acquisition of left and right-handed CPL images for enantioselective differential contrast microscopy, with a diffraction-limited spatial resolution (i.e. 126 nm lateral, 396 nm axial resolution using ×63 1.4 NA (numerical aperture) objective) across a typical field of view (FOV) of 100 × 100 µm in 9 s, when employing 355 nm single-photon activation with an Nd:YAG (3rd harmonic) laser. The CPL-LSCM could be a radical new tool in bio-imaging enabling the study of fundamental chiral interactions within live cells by harnessing the unique and uncharted power of CPL. In addition to cellular applications, CPL-LSCM could be used in studies of thin and thick film embedded CPL emitters, for applications such as physically unclonable multi-layered CPL-active security inks16,17, and next-generation organic light-emitting diodes18.

## Results

Throughout this work when discussing europium CPL, we selected the magnetic dipole (MD) allowed ΔJ = 1 transition (λ ~ 595 nm) because it exhibits both high overall emission intensity and a high gem value (i.e. an overall high CPL brightness) for the employed Eu:complexes. In this MD allowed transition manifold around 595 nm, europium complexes with transitions of the same sign of CPL emission have been identified. Therefore, using optical filters, the whole ΔJ = 1 manifold can be selected maximising light collection efficiency; it represents the best emission window to examine for Eu complexes in CPL-LSCM.

### Multi-photon (MP) CPL spectroscopy

CPL spectroscopy is a well-established discipline, with CPL emission maximised for emission transitions which are MD allowed and electric dipole (ED) forbidden. CPL emission is most commonly quantified in terms of the emission dissymmetry factor, $${g}_{{{{{\rm{em}}}}}}$$, calculated by

$${g}_{{{{{\rm{em}}}}}}=\,\frac{2({I}_{{{{{\rm{L}}}}}-{{{{{\rm{CPL}}}}}}}-\,{I}_{{{{{\rm{R}}}}}-{{{{{\rm{CPL}}}}}}})}{\left({I}_{{{{{\rm{L}}}}}-{{{{{\rm{CPL}}}}}}}+\,{I}_{{{{{\rm{R}}}}}-{{{{{\rm{CPL}}}}}}}\right)}.$$
(1)

Where I(L-CPL) and I(R-CPL) are the intensities of (left-handed) L-CPL and (right-handed) R-CPL emission; $${g}_{{{{{\rm{em}}}}}}$$ = 2 indicates 100% L-CPL emission, $${g}_{{{{{\rm{em}}}}}}$$ = −2 indicates 100% R-CPL emission, and $${g}_{{{{{\rm{em}}}}}}$$ = 0 indicates net-zero circular polarisation. The strongest CPL signals to date have been generated by lanthanide coordination complexes, specifically europium complexes, exhibiting $${g}_{{{{{\rm{em}}}}}}=|1.38|$$ for single complexes and $${g}_{{{{{\rm{em}}}}}}=\left|1.45\right|$$ for chiral supramolecular polymers19,20. Recently, the more comprehensive metric of circularly polarised brightness (CPB) has been introduced16,21. CPB serves as a metric for the total number of circularly polarised photons emitted and combines the molar absorption coefficient (ξabs), quantum yield ($$\phi$$em), and $${g}_{{em}}$$. CPB is calculated as

$${{{{{\rm{CPB}}}}}}={{{{{{\rm{\xi }}}}}}}_{{{{{{\rm{abs}}}}}}}{\phi }_{{{{{{\rm{em}}}}}}}({g}_{{{{{\rm{em}}}}}}/2)$$
(2)

It has units of cm−1 M−1. A wide variety of CPL emitting molecular systems can produce useable CPB values (loosely defined here as ~>50 cm−1 M−1), including BODIPYs, helicenes, excimers, cyclophanes, and d-metal complexes21. However, for the purposes of CPL-LSCM, chiral lanthanide complexes are pre-eminent owing to their excellent photophysical properties: large Stokes’ shifts, narrow, line-like emission spectra, tunable emission and excitation properties, intricate CPL emission, with the potential for exceptional $${g}_{{{{{\rm{em}}}}}}$$ and CPB values (e.g. CPB values of >1000 and >3000 cm−1 M−1 with europium complexes)5. However, CPL spectroscopy to date has been concerned with single-photon excitation, which is sub-optimal for cellular imaging studies due to the associated potential photo-damage and shallow tissue penetration of near-UV excitation.

Multiphoton (MP) spectroscopy and microscopy techniques reduce cellular phototoxicity by harnessing a tightly focused low-energy near infra-red (NIR) laser pulse (typically femtoseconds) to stimulate emission from fluorescent/luminescent molecules that would otherwise require absorption of a single high-energy UV photon22. The tightly defined spatial constraints of MP microscopy offers both improved axial (z-axis) resolution and sub-cellular sectioning capability for imaging and photodynamic therapy applications23. However, the field of MP-CPL has been largely unexplored. We are aware of just one previous report of an MP up-conversion-CPL spectrum in the literature of chiral perovskite nanocrystals24.

Two-photon excitation (2PE) CPL spectroscopic studies of a europium (III) complex were undertaken by coupling a tunable femtosecond pulsed laser (680–1300 nm, Coherent Discovery TPC, 100 fs, 80 MHz) to two pre-existing CPL spectrometers. (1) a conventional PEM25 CPL spectrometer, and (2) a next-generation solid-state CCD (SS-CCD) CPL spectrometer15. Either approach yielded the same CPL spectrum, measuring a model CPL complex, modified Eu:BPEPC (Eu[(4-methoxyphenyl)alkynyl-bpepc]3}Cl3 Fig. 1)26, but as per previous publications, the SS-CCD-CPL spectrometer acquired the CPL spectrum 800 times faster than the PEM-CPL spectrometer (under 10 s for a 1000 accumulation spectrum). For the purposes of this work, we will report 2PE-CPL spectra from the PEM CPL spectrometer because this form of CPL spectrometry represents the current benchmark instrumentation of the CPL spectroscopy community.

For efficient two-photon excitation, a material must have a high two-photon absorption (TPA, 2PA) cross-section ($${\sigma }_{2}$$) (GM) with a favourable emission quantum yield. Therefore, we extend CPB to two-photon-activation CPB (2PE-CPB or CPB2PE) as

$$2{{{{{\rm{PE}}}}}}-{{{{{\rm{CPB}}}}}}={\sigma }^{2}\times {\phi }_{{em}}\times \frac{{g}_{{{{{\rm{em}}}}}}}{2}$$
(3)

Certain lanthanide complexes (especially those of Eu(III) and Tb(III)) have adequate two-photon cross-sections27, leading to good 2PE-CPB values, paving the way towards two-photon activated live-cell CPL-LSCM. We determined the cross-sections (σ2), of the standard materials (modified Eu:BPEPC and Eu:L1) discussed herein26,28, according to established procedures (see SI)27,29. It is important to note that due to the nonlinear effect of 2PE (non-degenerate two-photon absorption) the 2PE wavelength is often lower and extremely rarely double of the 1PE absorption maximum. Due to the quadratic relationship between the intensity of the 2PE excitation and the triggering of a fluorescent event the shape of 2PE excitation is inherently always far narrower, sharper too than that of the 1PE excitation23,29.

We verified that the MP excitation process was a two-photon event by recording an excitation power dependence; confirmed by the resulting line having a slope of ~2 on a logarithmic scale (see Fig. 1A). We measured the MP cross-section of the recently developed CPL-standard Eu(III)-complex, (modified Eu:BPEPC) via these methods (Fig. 1). Its 2PE cross-section was determined to be σ2 = 142 ± 3 and 147 ± 3 GM (1 GM = 10−50 cm4 s photon−1) for the Λ- and Δ-enantiomers in methanol (MeOH), respectively. This result is particularly notable because MP cross-sections have not previously been determined for enantiomers of CPL active materials. Eu:L1, is a complex which has shown enantioselective localisation in live-cell experiments27,30. The MP cross-section of Eu:L1 in MeOH was determined to be σ2 = 51 ± 3 GM for both the Λ- and Δ-enantiomers (see SI Fig. 1).

### Enantioselective CPL-LSCM microscopy imaging

Details of the CPL-LSCM set-up are shown in Fig. 2. In brief, light from the sample plane of the LSCM exits the microscope via an output port and into an external CPL analysis module, which is adapted from the rapid CPL spectrometer that we recently reported15. First, the waveband of interest is selected by a switchable band-pass filter. Then, an achromatic wave plate converts left and right circularly polarised light into orthogonal linearly polarised states. The light is then split into two analysis pathways by a 50:50 beam-splitter cube. The two linear polarised light states generated (horizontal and vertical polarisation) corresponding to left or right CPL are selected by a carefully aligned linear polarizer, housed in a high-precision computer-controlled rotation mount15. The emission intensity of each pixel is quantified in a conventional LSCM scanned manner by a dedicated high sensitivity avalanche photodiode pair. Whilst each detection arm can operate independently, both components are matched in alignment and specification to enable rapid and simultaneous acquisition of left and right CPL images. Full technical details of the CPL-LSCM system and the applied image processing methodology are provided in the Supporting information.

EDCC imaging was realised by subtraction of the simultaneously recorded left-handed CPL image from the right-handed CPL (and vice versa) using ImageJ software (v1.49)31.

To demonstrate the CPL-LSCM on well-controlled targets, we first re-created the paper test-target [Test Target 1] which had been used for the proof-of-concept CPL microscopy studies reported in 20169. This was achieved by simply depositing 15 μL of enantiopure solutions of Eu:L1 (10−4 M) in MeOH onto the commercially available optical brightener-free paper substrate from Canson®, allowing the sample to dry at room temperature. This procedure replicated the results obtained with the epifluorescence microscope and further demonstrated the excellent performance of the CPL-LSCM. The experiment revealed differences arising from the texture of the brightener-free paper. Under the applied ×40 (0.7 NA, air) magnification, it was found that the paper has a ‘rough’ and ‘smooth’ side, which was not observed in prior studies with the epifluorescence CPL microscope (see SI Figs. 46 and 8)9. To remove the variables introduced by the paper substrate, another test-target was developed [Test Target 2] where enantiopure solutions of Eu:L1 (5 × 10−5 M) were deposited into a uniform polymer matrix (Polyvinylpyrrolidone (PVP-40), Sigma-Aldrich)9,28 by spin-coating on glass substrates (170 µm thick standard microscope coverslips). Distribution of the complexes within a polymer matrix is of particular interest for ultra-secure anti-counterfeiting CPL-active security ink applications (e.g. for application within plastic banknotes) and solution-processed CPL-OLEDs.

To demonstrate that Eu:L1 retains its distinctive emission properties within the PVP40 polymer, we measured CPL emission, 2PE-CPL emission, and 2PE-cross-section measurements of Eu:L1 in anhydrous N-methyl-2-pyrrolidone (NMP) (see Fig. 3). NMP was selected because NMP is structurally almost identical to the monomer unit of PVP polymers (N-Vinylpyrrolidone). This is crucial because it has recently been reported that CPL signal intensity and even CPL sign may vary as a function of solvent or medium polarity32. We found that the CPL signal intensity (|gem| and CPB) and sign were unaltered and the 2PE cross-section of Eu:L1 was even slightly enhanced in NMP (σ2 = 73 ± 3 GM for Λ- and Δ-enantiomer) compared to MeOH (σ2 = 51 ± 3 GM for Λ- and Δ-enantiomer), validating our choice of host polymer for spin-coated test targets.

However, the non-uniform edges of the glass substrates caused light helicity inversion at the edges of the glass substrates owing to unwanted internal reflection, making them less than ideal for side-by-side demonstration of enantioselective CPL-LSCM. This behaviour is ascribed to dramatically reduced gem values observed from Test Target 2 as a result of reflected light-induced CPL helicity inversion (see SI Figs. 7 and 8).

A third test target was therefore developed with improved properties [Test Target 3]. This was achieved by heating a glass microscope slide to 35 °C on a hot plate, and drop-casting 100 µL of solutions of the Λ- and Δ-enantiomers (10−4 M) 1:1 v/v Eu:L1:PVP40 solutions in MeOH side-by-side onto the slide using a multi-channel pipette. The slide was dried on the hot plate for 1 min, removed and allowed to dry at room temperature for 5 min9.

Test Target 3 was successfully used during validation of the CPL-LSCM setup and provided superior quality diffraction-limited images (see Fig. 4 and SI Fig. 7). Simultaneous enantioselective imaging was thereby achieved in the same FOV using bright CPB CPL emitters in a validated and controlled test target of enantiopure lanthanide complexes as homogenous thin film deposits (from a 210 × 210 × 2 µm FOV). Additionally, we measured the total CPL spectrum of the Test Target 3 using the PEM-CPL spectrometer (see SI Figs. 2 and 3), showing excellent correspondence with respect to both CPL sign and CPB.

### Enantioselective CPL-LSCM of live cells

To demonstrate the live-cell imaging capabilities of the newly constructed CPL-LSCM, NIH 3T3 (mouse skin fibroblast, ATCC-CRL-1658) cells were dosed with 30 μM of enantiopure Λ- and Δ-Eu:L1 complex for 14 h as per Frawley et al.28. The images in Fig. 5 demonstrate that CPL-LSCM can simultaneously collect images and differentiate between the left- and right-handed CPL emission arising from the cells. The enantiomers of Λ- and Δ-Eu:L1 appeared to localise to different organelles with well-resolved brightness differences observable within NIH 3T3 cells.

To investigate further the enantioselective localisation of Λ- and Δ-Eu:L1, we repeated this experiment with the addition of LysoTrackerTM DND-26 Green and MitoTrackerTM FM Green dyes. From the differential CPL-LSCM images (Fig. 6), it can be seen that the Δ-enantiomer strongly overlaps with the emission from LysoTrackerTM DND-26 Green (Pearson’s-coefficient = 0.89, Fig. 6E), whereas the Λ-enantiomer strongly overlaps with that of MitoTrackerTM FM Green (Pearson’s-coefficient = 0.94, Fig. 6J). Without enantioselective differential CPL imaging, these coefficients are significantly reduced (0.69 and 0.73, Fig. 6D, I, respectively).

This study unequivocally demonstrates and confirms that the different enantiomers Eu:L1 selectively target different cellular organelles. Enantioselective imaging is a significant milestone in live-cell optical microscopy. The above detailed simple modifications to any existing LSCM enable researchers worldwide to exploit the importance and versatility of chiral bioimaging. This could trigger a paradigm shift in the fields of molecular cell biology and chemistry, opening new avenues in bioprobe research by enantioselectively targeting and tracking chiral species.

## Discussion

To conclude, we have presented three major advances in the intertwined disciplines of CPL spectroscopy and chiral luminescence imaging. Firstly, we have demonstrated the CPL-LSCM system, which is capable of rapidly and simultaneously acquiring diffraction-limited enantioselective chiral-contrast based CPL-differential images for the sub-cellular tracking of emissive chiral sub-cellular probes. This milestone is accompanied by the proof-of-concept demonstration of 2PE-CPL spectroscopy, showing that low-energy 2PE-CPL-LSCM is ripe for future development. Secondly, we have created a well-controlled inert CPL test target for use as a standard for enantioselective chiral-contrast imaging. This test target consists of enantiopure solutions of a suitable europium complex simultaneously drop-cast in a spatially separated manner directly onto conventional glass microscope slides. This simple test target can serve to compare and benchmark future enantioselective chiral-contrast CPL differential imaging systems that may be developed by the multi-disciplinary imaging community. Thirdly, we have imaged Λ- and Δ-enantiomers of a known chiral europium complex that localises to different organelles within mouse skin fibroblast (NIH 3T3) cells, with each enantiomer showing an excellent co-localisation profile with common lysosomal and mitochondrial tracker dyes.

We anticipate that these developments will open uncharted research avenues for fundamental studies of chiral interactions in the domains of chemistry and molecular biology. CPL-LSCM will be a vital new tool in optical microscopy aiding the development of chiral bio-probes to be taken to the next level. In material sciences, CPL-LSCM could be used for characterising 3D display technologies (e.g. emissive chiral polymers) and verification of physically unclonable stochastically micro-patterned CPL-active security inks16,17,18. Ultimately, the work presented here opens a new window into the world of chiral molecular interactions which is ripe for exploration by shedding light on the previously unexploited chiral biochemical processes that fundamentally underpin life.

## Methods

### EDCC imaging

Microscope control and image acquisition and analysis were performed with Leica’s commercial microscope software LAS-X. EDCC imaging is achieved using ImageJ software (v1.49)31, with its built-in image calculator add-on software by subtracting one CPL channel from the other, and vice versa. The convention used herein is: left-handed enantioselective contrast = left CPL—right CPL. Right-handed enantioselective contrast = right CPL—left CPL. Images for a typical 1024 × 1024 pixel FOV with 10 line accumulation bidirectional scanning sequence were typically acquired in 90 s (corresponding to 10 full-frame accumulations). Confocality—axial (z) resolution—was governed by the applied pinhole diameter denoted in Airy disk units to preserve resolution and maximise light detection from the FOV.

Images were obtained using the detector saturation mode of LAS-X where each image is assessed for maximum intensity value. Each image is only recorded if no 4 × 4 pixel cluster (Nyquist sampling covering an area determined by the systems optical resolution, 126 × 126 nm at 355 nm excitation using 1.4 NA objective) possesses average intensity values of 255 on an 8-bit greyscale. This allows the employed gain of each detector to be synchronised and kept constant, so no error associated with pixel intensity saturation is included accidentally contributing to pixel uncertainties, lowering S/N and exponentially increasing the limit of detection values.

Non-live cell 8-bit average pixel chiroptical contrast value calculations were facilitated by selecting and averaging five different positions non-overlapping equal size and shape arbitrary area of the sample with respect to each enantiomer and dark background. Due to the 1024 × 1024 pixel size of each recorded image total FOV, this arbitrary area has been kept at a constant area of 100 × 100 pixels region of interest (ROI). The average maximum 8-bit grayscale pixel intensity values were determined using the LSCM’s built-in LAS-X software that is employing a maximum average value ROI histogram methodology that is based on standard Gaussian distribution profiling of the average intensity values. Due to the employed methodology and the averaging nature of image acquisition and ROI calculation the limit of detection (error associated with) 8-bit greyscale contrast value is below 1% (<3 average greyscale value on a 0–255 pixel intensity scale).

During live-cell imaging, adaptations of the above detailed chiroptical contrast greyscale value determination methodology were applied. In this case, full FOV 8-bit contrast values have been calculated using the LAS-X software. To eliminate errors associated with the number of cells occupying the FOV—in other words, the variable amount of dark ‘black’ background in each image, this value has been corrected with a below limit of detection value correction. In each case, the software only uses pixel for the average 8-bit grayscale intensity value determines if the intensity value of the pixel is above the value of 4 (on a 0–255 pixel intensity scale). This is determined using the total Europium emission image and the selected arbitrary ROI area selection is then kept identical throughout the imaging sequence resulting in high precision chiroptical contrast calculations.

Pearson correlation coefficients were calculated following standardised protocols using the corresponding channel of the colour split raw images using the ImageJ—JACoP plug in33.

### Statistics and reproducibility

Where instruments incorporating a scanning monochromator have been used (absorption, emission, and excitation spectra) each sample have been recorded and averaged as triplicate measurements. Spectra, where CCD detectors have been employed, such as two-photon cross-section determination, multiphoton and CPL spectroscopy, have been measured as an average of a thousand spectra on triplicate samples.

Microscopy images presented herein are representative images of the experiments discussed. Each experiment has been repeated in triplicates and each sample has been recorded and studied recording a minimum of five separate imaging sequences.

Imaging parameters presented, such as brightness and chiroptical contrast have been calculated on each individual imaging sequence according to the protocol detailed in the Methods and the Supplementary Information (SI) section.

### Reporting summary

Further information on research design is available in the Nature Research Reporting Summary linked to this article.

## Data availability

All data generated and analysed, including spectra and raw microscopy images, during this study are available from the corresponding author upon request.

## Code availability

Custom codes are written in Labview2013 and Matlab2019b developed and used during this study are available from the corresponding author upon request.

## References

1. Blackmond, D. G. The origin of biological homochirality. Cold Spring Harb. Perspect. Biol. 2, a002147–a002147 (2010).

2. Tokunaga, E., Yamamoto, T., Ito, E. & Shibata, N. Understanding the thalidomide chirality in biological processes by the self-disproportionation of enantiomers. Sci. Rep. 8, 6–12 (2018).

3. Singh, J. & Hagen, T. J. Chirality and Biological Activity. in Burger’s Medicinal Chemistry and Drug Discovery (John Wiley & Sons, Inc., 2010). https://doi.org/10.1002/0471266949.bmc016.pub2.

4. Yamada, T. et al. Synthesis of chiral Labtb and visualization of its enantiomeric excess by induced circular dichroism imaging. Chemistry 25, 6698–6702 (2019).

5. Zhou, Y., Li, H., Zhu, T., Gao, T. & Yan, P. A highly luminescent chiral tetrahedral Eu4L4(L′)4 cage: chirality induction, chirality memory, and circularly polarized luminescence. J. Am. Chem. Soc. 141, 19634–19643 (2019).

6. Mawatari, K., Kubota, S. & Kitamori, T. Sensitive chiral analysis method for microchip by circular dichroism UV thermal lens microscope (UV-CD-TLM). Micro Total Anal. Syst. 78, 1582–1584 (2006).

7. Narushima, T. & Okamoto, H. Circular dichroism microscopy free from commingling linear dichroism via discretely modulated circular polarization. Sci. Rep. 6, 1–10 (2016).

8. Doistau, B., Jiménez, J.-R. & Piguet, C. Beyond chiral organic (p-block) chromophores for circularly polarized luminescence: the success of d-block and f-block chiral complexes. Front. Chem. 8, 1–27 (2020).

9. Frawley, A. T., Pal, R. & Parker, D. Very bright, enantiopure europium(III) complexes allow time-gated chiral contrast imaging. Chem. Commun. 52, 13349–13352 (2016).

10. Miller, T. L. et al. Calcium binding sites of rabbit troponin and carp parvalbumin. FEBS Lett. 58, 1–3 (1975).

11. Brittain, H. G. & Richardson, F. S. Circularly polarized emission studies on the chiral nuclear magnetic resonance lanthanide shift reagent tris(3-trifluoroacetyl-d-camphorato)europium(III). J. Am. Chem. Soc. 1, 5858–5863 (1976).

12. Tsumatori, H., Harada, T., Yuasa, J., Hasegawa, Y. & Kawai, T. Circularly polarized light from chiral lanthanide(III) complexes in single crystals. Appl. Phys. Express 4, 011601 (2011).

13. Koike, H., Nozaki, K. & Iwamura, M. Microscopic imaging of chiral amino acids in agar gel through circularly polarized luminescence of Eu III complex. Chemistry 15, 85–90 (2020).

14. Schermelleh, L., Heintzmann, R. & Leonhardt, H. A guide to super-resolution fluorescence microscopy. J. Cell Biol. 190, 165–175 (2010).

15. MacKenzie, L. E., Pålsson, L.-O., Parker, D., Beeby, A. & Pal, R. Rapid time-resolved circular polarization luminescence (CPL) emission spectroscopy. Nat. Commun. 11, 1676 (2020).

16. MacKenzie, L. E. & Pal, R. Circularly polarized lanthanide luminescence for advanced security inks. Nat. Rev. Chem. https://doi.org/10.1038/s41570-020-00235-4 (2020).

17. Arppe, R. & Sørensen, T. J. Physical unclonable functions generated through chemical methods for anti-counterfeiting. Nat. Rev. Chem. 1, 0031 (2017).

18. Wan, L. et al. Inverting the handedness of circularly polarized luminescence from light-emitting polymers using film thickness. ACS Nano 13, 8099–8105 (2019).

19. Lunkley, J. L., Shirotani, D., Yamanari, K., Kaizaki, S. & Muller, G. Chiroptical spectra of a series of tetrakis((+)-3-heptafluorobutylyrylcamphorato)lanthanide(III) with an encapsulated alkali metal ion: circularly polarized luminescence and absolute chiral structures for the Eu(III) and Sm(III) complexes. Inorg. Chem. 50, 12724–12732 (2011).

20. Kumar, J., Marydasan, B., Nakashima, T., Kawai, T. & Yuasa, J. Chiral supramolecular polymerization leading to eye differentiable circular polarization in luminescence. Chem. Commun. 52, 9885–9888 (2016).

21. Arrico, L., Di Bari, L. & Zinna, F. Quantifying the overall efficiency of circularly polarized emitters. Chemistry 27, 2920–2934 (2021).

22. Denk, W., Strickler, J. H. & Webb, W. W. Two-photon laser scanning fluorescence microscopy. Science 248, 73–76 (1990).

23. Liu, D. et al. Near-infrared light activates molecular nanomachines to drill into and kill cells. ACS Nano 13, 6813–6823 (2019).

24. Chen, W. et al. Two-photon absorption-based upconverted circularly polarized luminescence generated in chiral perovskite nanocrystals. J. Phys. Chem. Lett. 10, 3290–3295 (2019).

25. Bruce, J. I., Parker, D., Lopinski, S. & Peacock, R. D. Survey of factors determining the circularly polarised luminescence of macrocyclic lanthanide complexes in solution. Chirality 14, 562–567 (2002).

26. Starck, M., MacKenzie, L. E., Batsanov, A. S., Parker, D. & Pal, R. Excitation modulation of Eu:BPEPC based complexes as low-energy reference standards for circularly polarised luminescence (CPL). Chem. Commun. 55, 14115–14118 (2019).

27. Xu, C. & Webb, W. W. Measurement of two-photon excitation cross sections of molecular fluorophores with data from 690 to 1050 nm. J. Opt. Soc. Am. B 13, 481 (1996).

28. Frawley, A. T., Linford, H. V., Starck, M., Pal, R. & Parker, D. Enantioselective cellular localisation of europium (III) coordination complexes. Chem. Sci. 9, 1042–1049 (2018).

29. Pålsson, L.-O., Pal, R., Murray, B. S., Parker, D. & Beeby, A. Two-photon absorption and photoluminescence of europium based emissive probes for bioactive systems. Dalt. Trans. https://doi.org/10.1039/b710717j (2007).

30. Makarov, N. S., Drobizhev, M. & Rebane, A. Two-photon absorption standards in the 550-1600 nm excitation wavelength range. Opt. Express 16, 4029 (2008).

31. Schneider, C. A., Rasband, W. S. & Eliceiri, K. W. NIH Image to ImageJ: 25 years of image analysis. Nat. Methods 9, 671–675 (2012).

32. Fradgley, J. D., Frawley, A. T., Pal, R. & Parker, D. Striking solvent dependence of total emission and circularly polarised luminescence in coordinatively saturated chiral europium complexes: solvation significantly perturbs the ligand field. Phys. Chem. Chem. Phys. 23, 11479–11487 (2021).

33. Bolte, S. & Cordelières, F. P. A guided tour into subcellular colocalization analysis in light microscopy. J. Microsc. 224, 213–232 (2006).

## Acknowledgements

R.P. acknowledges support from the Royal Society University Research Fellowship URF\R\191002 and H2020-MSCA-ITN-859752 HEL4CHIROLED. R.P. and P.S. acknowledge support from BBSRC BB/S017615/1, L.M. acknowledges support from the BBSRC Discovery Fellowship BB/T009268/1. P.S. would like to thank Dr. Piotr Pander for his assistance with spin-coating. R.P. thanks Prof. Andrew Beeby for the stimulating discussions regarding CPL spectroscopy. D.P. thanks Dr. Matthieu Starck and Dr. Andrew Frawley for the synthesis of Eu complexes used herein. We are also thankful for the ongoing support of Leica Microsystems UK (Dr. Malcolm Lang, Brian Preston and Jason Lewis) and Coherent UK (Graham Wright and Blair Welsh).

## Author information

Authors

### Contributions

P.S.:1 Co-constructed the CPL-LSCM performed all blotting and casting experiments and drafted/edited the paper. L.M.:1 Co-constructed the CPL-LSCM, Co-designed SS-CPL and edited the paper. D.P.: Secured funding for the proof-of-concept epifluorescence microscope with R.P., provided lanthanide complexes for analysis and edited the paper. R.P.: Secured project funding, designed and constructed the confocal CPL microscope, performed multi-photon and live-cell experiments, and drafted/edited the paper. 1Co-first authors can prioritise their names when adding this paper’s reference to their resumes.

### Corresponding author

Correspondence to Robert Pal.

## Ethics declarations

### Competing interests

R.P. is an inventor on patent WO2016174395A1: Light detecting apparatus for simultaneously detecting left- and right-handed circularly polarised light. The authors declare no competing interests.

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Stachelek, P., MacKenzie, L., Parker, D. et al. Circularly polarised luminescence laser scanning confocal microscopy to study live cell chiral molecular interactions. Nat Commun 13, 553 (2022). https://doi.org/10.1038/s41467-022-28220-z

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• DOI: https://doi.org/10.1038/s41467-022-28220-z