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Achieving λ/10 Resolution CW STED Nanoscopy with a Ti:Sapphire Oscillator

  • Yujia Liu,

    Affiliations School of Biomedical Engineering, Shanghai Jiao Tong University, Shanghai, China, Department of Biomedical Engineering, College of Engineering, Peking University, Beijing, China

  • Yichen Ding,

    Affiliation Department of Biomedical Engineering, College of Engineering, Peking University, Beijing, China

  • Eric Alonas,

    Affiliation Wallace H Coulter Department of Biomedical Engineering, Georgia Institute of Technology and Emory University, Atlanta, Georgia, United States of America

  • Wenli Zhao,

    Affiliation College of Life Sciences, Peking University, Beijing, China

  • Philip J. Santangelo,

    Affiliation Wallace H Coulter Department of Biomedical Engineering, Georgia Institute of Technology and Emory University, Atlanta, Georgia, United States of America

  • Dayong Jin,

    Affiliation Advanced Cytometry Labs, MQphotonics Research Centre, Macquarie University, Sydney, New South Wales, Australia

  • James A. Piper,

    Affiliation Advanced Cytometry Labs, MQphotonics Research Centre, Macquarie University, Sydney, New South Wales, Australia

  • Junlin Teng,

    Affiliation College of Life Sciences, Peking University, Beijing, China

  • Qiushi Ren,

    Affiliations School of Biomedical Engineering, Shanghai Jiao Tong University, Shanghai, China, Department of Biomedical Engineering, College of Engineering, Peking University, Beijing, China

  • Peng Xi

    xipeng@pku.edu.cn

    Affiliation Department of Biomedical Engineering, College of Engineering, Peking University, Beijing, China

Achieving λ/10 Resolution CW STED Nanoscopy with a Ti:Sapphire Oscillator

  • Yujia Liu, 
  • Yichen Ding, 
  • Eric Alonas, 
  • Wenli Zhao, 
  • Philip J. Santangelo, 
  • Dayong Jin, 
  • James A. Piper, 
  • Junlin Teng, 
  • Qiushi Ren, 
  • Peng Xi
PLOS
x

Abstract

In this report, a Ti:Sapphire oscillator was utilized to realize synchronization-free stimulated emission depletion (STED) microscopy. With pump power of 4.6 W and sample irradiance of 310 mW, we achieved super-resolution as high as 71 nm. With synchronization-free STED, we imaged 200 nm nanospheres as well as all three cytoskeletal elements (microtubules, intermediate filaments, and actin filaments), clearly demonstrating the resolving power of synchronization-free STED over conventional diffraction limited imaging. It also allowed us to discover that, Dylight 650, exhibits improved performance over ATTO647N, a fluorophore frequently used in STED. Furthermore, we applied synchronization-free STED to image fluorescently-labeled intracellular viral RNA granules, which otherwise cannot be differentiated by confocal microscopy. Thanks to the widely available Ti:Sapphire oscillators in multiphoton imaging system, this work suggests easier access to setup super-resolution microscope via the synchronization-free STED.

Introduction

Fluorescence microscopy has become an essential tool to study biological molecules, pathways and events in living cells, tissues and animals. Its key advantages over other forms of microscopy arise from the use of specific, minimally invasive molecular staining and compatibility with living cells. Fluorescence microscopes with the most advanced confocal geometries available yield optical resolution approaching the theoretical Abbe diffraction limit of ∼ 200 nm, but this is still larger than many subcellular structures, which are too small to be observed in detail. These limitations have driven the development of super-resolution optical imaging methodologies over the past decade, and have significantly impacted many fields of science [1], [2], [3], [4], [5].

Bypassing the optical diffraction limit in far-field optical microscopy has been realized by two key pioneering concepts: spatially patterned excitation with emission inhibition, such as Stimulated Emission Depletion (STED) microscopy [6], [7], [8] and Saturated Structured Illumination Microscopy (SSIM) [9], [10]; and high-precision localization of single fluorophores through individual activation, such as STochastic Optical Reconstruction Microscopy (STORM) [11], [12] and Photo-Activated Localization Microscopy (PALM) [13]. Stimulated Emission Depletion (STED) was the first and most direct approach to overcoming the diffraction limit for far-field nanoscopy. STED microscopy uses an intense doughnut-shaped beam surrounding the excitation focus to switch the fluorophore(s) in the sample to a “dark” state through stimulated emission. This effectively eliminates the periphery of the Point Spread Function (PSF), resulting in a narrower PSF, or super-resolution.

The depletion efficiency of STED can be optimized with the pulsed excitation and the temporal delayed pulsed STED beam [7]. This requires precise synchronization of two laser pulses and maintenance of the accurate time delay [14], [15], [16], [17], [18], [19], [20]. To meet these requirements, either a laser diode was specially designed with a rather sophisticated optical or electrical delay line [14], [15], [16], [17], [18], or a single laser was used to generate both excitation and STED pulses to minimize synchronization steps [19], [20]. Continuous Wave (CW) STED, with both excitation and STED beams in CW mode, can be engineered based on spectral discrimination of the spontaneous emission and stimulated emission of the fluorescent molecules, and has been successfully applied to image neurofilaments in neuroblastoma cells [21], syntaxin clusters in the cell membrane [21], the nuclear lamina of mammalian cells [21], and the endoplasmic reticulum of living cells [22]. CW STED is beneficial because it is synchronization-free, and requires no pulse length or timing optimization for the excitation and depletion beams. This characteristic makes it easier to adapt to a conventional confocal fluorescence configurations. Previous reports of CW STED utilized either high pump power laser systems [21], or the combination of multiple fiber lasers [22]. However, these lasers are not readily available in biomedical instrumentation labs, which might explain their limited use. The only other current option for CW STED are commercial microscopes, but these are prohibitively expensive for most users.

On the other hand, the Ti:Sapphire laser has recently been used as both an excitation and depletion source in a two-photon STED system for super-resolution neuron imaging [23]; as well as for single-laser, single-wavelength STED nanoscopy [24]. The work presented here further expands the application of Ti:Sapphire lasers to STED nanoscopy.

In this paper, we demonstrated a synchronization-free CW STED microscope using a 6 Watt Diode-Pumped Solid State (DPSS) 532 nm laser pumped Ti:Sapphire oscillator tuned to CW mode, which is a source broadly available in many two-photon microscope systems [25], [26], [27], [28], [29]. Taking advantage of the wavelength tunability of the Ti:Sapphire laser, the depletion wavelength was optimized for different dyes. Using this system we demonstrated a super-resolution of 71 nm, and resolved the fine structures of actin filaments, intermediate filaments, and microtubules. In situations where optical deconvolution fails to interpret the structure of aggregated nanospheres, CW STED can correctly discern the nanospheres with ∼200 nm distance. Interestingly, a pair of parallel actin filaments, 240 nm from each other, was clearly imaged with STED, which could be misinterpreted as with a double-helix structure in confocal microscopy due to the lack of sufficient resolution. Furthermore, we applied the CW STED for the first time to visualize the viral genomic RNA of human respiratory syncytial virus (hRSV) in HEp-2 cells resulting in a high-resolution image clearly showing individual RNA granules. Moreover, we demonstrated the utility of Dylight 650 as a far-red dye suitable for STED microscopy with improved depletion efficiency.

Results

Figure 1 illustrates the schematic setup and preliminary evaluation of the stimulated emission depletion efficiencies on different fluorescent dyes (1d). We employed a vortex 0–2π phase plate to generate the doughnut shaped depletion beam for de-exciting the fluorescence by stimulated emission [30]. As the resolution is determined by the depletion efficiency, not the diffraction limit, we first studied the effect of the depletion ratio on the spontaneous fluorescence by overlapping the STED focus (without phase modulation) with the excitation focus [31]. As shown in Figure 1d, the saturation intensity (in which the possibility of spontaneous emission and stimulated emission is equal) is measured to be ∼17 MW/cm2 for crimson beads at 763 nm, ∼14.4 MW/cm2 for DyLight 650 at 783 nm and ∼23.8 MW/cm2 for ATTO 647N at 763 nm (the intensities are measured before the 100x objective). The saturation intensity for ATTO647N is larger than previous literatures [21], [24], which may due to residual system optical aberration as well as the measurement condition, to which the extinction ratio of is insensitive. The reciprocal fitting of agrees well with the experimental data. When the STED beam was switched off, the system functioned as a normal confocal system, which was used to obtain data for comparison.

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Figure 1. Schematic of the CW STED system for far-field super-resolution optical nanoscopy.

The green line represents the excitation 635 nm laser, red line is the CW Ti: Sapphire STED beam, and the yellow line represents the fluorescence signal. SMF: single mode fiber; MMF: multi-mode fiber; DC1 and DC2 are dichotic filters. VPP: vortex 0–2π phase plate; QWP: quarter waveplate. The excitation PSF (a), doughnut depletion PSF overlapped with excitation PSF (b), and STED PSF (c) clearly shows the process of achieving super-resolution. Scale bar: 500 nm. The modulation efficiency versus the depletion intensity was measured with crimson beads, DyLight 650 and ATTO 647N solution (d). The STED wavelengths are 763 nm for crimson beads and ATTO 647N, and 783 nm for DyLight 650.

https://doi.org/10.1371/journal.pone.0040003.g001

The resolution of the prototype STED system was evaluated by imaging 20 nm crimson nanospheres. As shown Figure 2, at the maximum available STED power of 340 mW, the FWHM spot size was measured as small as 63 nm laterally, indicating an effective resolution of 59 nm after accounting for the size of the nanosphere [21]. With a total 20 nanospheres measured in the focal plane, the average resolution was calculated as 71 nm ±9 nm. This is in good agreement with the theoretical prediction of . The pixel dwell time is set to 0.2 ms in all the presented images.

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Figure 2. Confocal and corresponding CW-STED images of fluorescent 20-nm-diameter nanospheres.

(a) Confocal; (b) CW-STED; (c) The profile along the dashed line in (a) and (b) exhibits a spot size of 63 nm, indicating an effective resolution of ∼59 nm after subtraction of the bead size. Scale bar: 500 nm.

https://doi.org/10.1371/journal.pone.0040003.g002

Figure 3 shows images of the 200 nm nanospheres on glass. Adjacent nanospheres under the confocal system (a and c) can be clearly discriminated by the super-resolution CW STED system (b and d). Though the Richardson-Lucy (R-L) deconvolution algorithm can improve the resolution of both confocal and STED images (denoted confocal+ in a versus b, and STED+ in c versus d), once the adjacent nanospheres are within the optical diffraction limit, the STED+ (Fig 3d) can discern all the spheres clearly.

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Figure 3. Comparison of diffraction-limited confocal microscopy and STED nanoscopy for fluorescent 200-nm-diameter nanospheres.

(a) Confocal and (b) corresponding CW-STED images; (c) and (d) are the deconvolved results of (a) and (b). Scale bar: 500 nm.

https://doi.org/10.1371/journal.pone.0040003.g003

To demonstrate the resolving power of the CW STED nanoscope, all three cytoskeleton filaments were imaged: microtubules, intermediate filaments (keratin), and actin filaments. From the microtubule network of Vero cells, we can see that STED nanoscopy provides ∼128 nm FWHM with Dylight 650 staining (Figure 4). Because of the size of the microtubules is generally ∼25 nm, its junctions are hardly resolved with conventional microscope. However, with the STED, the fine microstructure can be visualized in Figure 4b, which result can be further improved by the R-L deconvolution in Figure 4c. In comparison, Figure 5 showed the images of the intermediate filament network in PtK2 cells, a male rat kangaroo kidney epithelial cell line stained with ATTO647N. The cross-sectional diameter is measured to be 168 nm on STED. The typical diameter of intermediate filament is ∼10 nm.

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Figure 4. Confocal, corresponding CW-STED, and deconvolved STED images of microtubules in a Vero cell stained with Dylight 650.

(a) Confocal; (b) CW-STED; (c) R-L deconvolution of (b). The intensity at the cross-section marked in (a), (b), and (c) inlets are plotted in (d). The wavelength and power density for the STED beam is 783 nm and ∼200 MW/cm2. Scale bar: 1 µm.

https://doi.org/10.1371/journal.pone.0040003.g004

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Figure 5. Confocal, corresponding CW-STED, and deconvolved STED images of keratin intermediate filaments in a PtK2 cell stained with ATTO 647N.

(a) Confocal; (b) CW-STED; (c) R-L deconvolution of (b). The intensity at the cross-section marked in (a), (b), and (c) boxed regions are plotted in (d). The wavelength and power density for STED beam is 763 nm and ∼200 MW/cm2. Scale bar: 1 µm.

https://doi.org/10.1371/journal.pone.0040003.g005

Furthermore, as reported by Oliva et al., insufficient resolution may lead to aliasing of image [32]. In our actin filament imaging of HeLa cell (Figure 6), we observed what appeared to be a single twisted actin filament from the confocal microscopy; this artifact was due to resolution larger than the size (∼8 nm) of filamentous actin and the lateral separation (∼240 nm) between filaments. However, with the aid of CW STED, we can clearly visualize the parallel structure of the actin filaments (Figure 6e).

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Figure 6. Confocal and corresponding CW-STED images of actin filaments in a HeLa cell.

(a) Confocal; (b) CW-STED. The boxed regions in (a) and (b) are magnified in (c) and (d), respectively. The intensities at the cross-section marked in (c) and (d) are plotted in (e). The wavelength and power density for the STED beam is 763 nm and ∼127 MW/cm2. Scale bar: 500 nm.

https://doi.org/10.1371/journal.pone.0040003.g006

RNA plays a critical role in mediating and regulating gene expression. Understanding RNA localization and dynamics will not only aid in our understanding of native cellular gene expression, but will also provide information on the life cycle of RNA viruses. Given that the size of most RNA molecules is often smaller than the diffraction limit, examining RNA localization is a model problem for the application of CW STED [33]. By utilizing exogenous multiply-labeled fluorescent probes described by Santangelo et al. [34], the genomic RNA of the human respiratory syncytial virus (hRSV strain A2) during cellular infection was specifically labeled with DyLight 650-conjugated probes and imaged via CW STED. As shown in Figure 7, a resolution of 82 nm on STED was achieved comparing to 290 nm on confocal. The contrast in performance is clearly obvious in Figure 7d and e where there is a higher concentration of RNA molecules.

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Figure 7. Confocal and corresponding CW-STED images of hRSV genomic RNA granules in a HEp2 cell.

Confocal (a) and corresponding CW-STED (b) results of isolated individual RNA, as well as RNA granules images by confocal (c) and CW-STED (d) are shown. The intensity at the cross-section marked in (d) and (e) are plotted in (c, f). The wavelength and power intensity for STED beam is 783 nm and ∼162 MW/cm2. Scale bar: 1 µm.

https://doi.org/10.1371/journal.pone.0040003.g007

Discussion

STED nanoscopy has been intensively investigated over the last decade, showing great promise for imaging cellular structures. It utilizes a donut depletion beam to de-excite fluorphoes at the edges of the excitation focus, thus breaking the diffraction limit. It can operate in either pulsed mode or CW mode.The pulsed mode can easily meet the depletion intensity requirements due to the high peak pulsed power, but the precise synchronization between the pulsed excitation laser and pulsed STED laser is both crucial and difficult to achieve and maintain. The successful demonstrations of synchronization-free CW STED, however, employed high power laser or a combination of multiple lasers [21], [22], which are not commonplace, thus limiting STED deployment. We report here a CW STED system with a Ti:Sapphire laser tuned to CW mode, and we achieved a super-resolution of 71 nm laterally, which is only one-tenth the emission wavelength. With super-resolution, the imaging of 200 nm nanospheres demonstrated that beads with distances beyond conventional resolution can be clearly discerned.

Two factors determine the resolution of CW STED nanoscopy: the saturation intensity of the fluorescence dye, and the depletion power applied. Here, for the first time, we have used Dylight 650 for STED nanoscopy and found that its saturation intensity is much lower than that of ATTO 647N, a commonly used STED fluorophore. This might lead to the exploration of other dyes that are more suitable for STED nanoscopy. The depletion power applied relates to two disadvantages associated with CW STED: (1) photobleaching is more pronounced due to constant excitation of the fluorophore and (2) photo-thermal damage to the specimen is possible due to the greater excitation energy applied over time. Therefore, the application of an anti-fade reagent, as well as mounting medium containing an oxygen scavenger, can improve the performance of CW STED imaging. Recent publications have reported that with the addition of Mowiol [21], [35], an oxygen scavenger system [35], [36], and reducing and oxidizing system [35], [37], the photostability of dye molecules can change dramatically. Therefore, it will be important in future studies to further characterize and optimize sample preparation protocols for each dye used in super-resolution nanoscopy..

Here, we have applied CW STED nanoscopy to all three cytoskeleton filaments (microtubule, intermediate filaments, actin filaments), whose sizes are smaller than the resolution of a diffraction-limit microscope, to demonstrate the performance of our STED system, and succeeded in discriminating parallel actin filaments, which appeared as a single structure by confocal imaging. We further demonstrated, for the first time, that STED nanoscopy can discern the Dylight 650-MTRIP-labeled viral RNAs in HEp-2 cells, with a resolution of 82 nm. The imaging capability of CW STED demonstrated in this report should help researchers interested in setting up their own STED systems with access to Ti:Sapphire oscillators, and to further apply STED nanoscopy to a broader, more diverse set of biological problems.

Materials and Methods

STED Instrumentation

The STED system was built based on a home-made confocal imaging system with 635 nm excitation. A Ti:Sapphire laser (Griffin-F, KMLabs, USA) pumped by a 6-Watt DPSS 532 nm laser (Finesse-6W, Laser Quantum, UK) was employed as the CW STED source. The output from the laser source is ∼800 mW. To generate the doughnut PSF for effective depletion, a vortex 0–2π phase plate (VPP-A, RPC Photonics) was used. We focused the beams into samples using an oil-immersion objective of NA = 1.4 (100x, PlanAPO, Zeiss). To obtain a 2-D image, a piezo scanning stage (Nanomax, Thorlabs) was employed to move the specimen. A photo-counting avalanche photodiode (SPCM-AQRH-13-FC, Perkin Elmer) was used to collect the fluorescence signal. The scanning and data collection were performed with a DAQ board (USB-6259, National Instruments), and image collection was accomplished with Imspector (Max-Plank Innovation).

Cells and Viruses

Vero cells (ATCC CCL-81) were maintained in High Glucose DMEM (Lonza) with 10% FBS (Hyclone), 100 U ml-1 penicillin, and 100 µg ml−1 streptomycin (Invitrogen). hRSV strain A2 (ATCC VR-1544) was propagated in HEp-2 cells (ATCC CCL-23) at a titer of 1×106 pfu/mL. Cells were plated the day before infection at 25% confluency. Cells were infected by removing the media, washing with PBS (without Ca2+ and Mg2+), adding virus at a multiplicity of infection (MOI) of 1, and incubating the cells for 1 h at 37°C. After adsorption, fresh medium was added to the inoculum.

Microtubule Immunofluorescence

Vero’s were plated the day before fixation at 25% confluency and were fixed with 100% methanol for 10 min at −20°C and additionally permeabilized with 100% acetone for 2 min at −20°C. Nonspecific antibody binding was blocked with 5% bovine serum albumin (EMD) in PBS for 30 min at 37°C. Veros were then incubated with a primary antibody against alpha tubulin (rabbit polyclonal IgG, Abcam ab18251) for 30 min at 37°C, washed twice in PBS, and incubated with a secondary antibody (goat anti-rabbit DyLight 650 IgG, Pierce) for 30 min at 37°C, washed twice in PBS, and mounted in a mixture of Mowiol 4–88 (Sigma) and DABCO (VWR) [38].

Keratin Immunofluoresnce

The PtK2 cells (a gift of Dr. K. Willig) were fixed with ice-cold methanol and blocked with BSA in PBS. The intermediate filaments were stained using indirect immunofluorescence. The primary antibody was a mouse anti-Keratin IgG (Dianova, DLN-09032), and the secondary antibody was a sheep anti-mouse IgG conjugated with ATTO 647N.

Actin Staining

HeLa cells were maintained in DMEM (Gibco) with 10% FBS (Hyclone). Cells were fixed with 100% methanol for 10 min at −20°C, washed twice in PBS. Cells were then incubated with Atto 647N-Phalloidin (ATTO-TEC) for 1h at room temperature, washed five times in PBS, and mounted in mixture of Mowiol 4–88 (Sigma) and DABCO (VWR).

hRSV Probe Delivery

To effectively image the genomic RNA of hRSV in HEp-2 cells, MTRIP probes labeled with DyLight 650 were made in a manner similar to [34]. Briefly, 2′-O-methyl RNA/DNA chimeric oligonucleotides, complimentary to the intergenic sites of the hRSV genomic RNA, with a 5′ biotin modification and 5 primary amine-C6 deoxy-thymines within the sequence, were labeled with DyLight 650 NHS Ester (Pierce), and filtered using a Zeba spin column (Pierce) to remove free dye. The labeled oligonucleotides were assembled into MTRIP probes and delivered into live cells using streptolysin O (SLO) at 48 h post infection, where they hybridized to multiple sites of the genomic RNA. Pores formed by SLO were closed via recovery in complete growth media for 30 minutes. This was followed by fixation in paraformaldehyde. Cells were mounted in a medium containing 80% glycerol, glucose, glucose oxidase, catalase, and β-mercaptoethanol [35].

Acknowledgments

The authors would like to acknowledge Dr. Katrin Willig, Dr. Benjamine Harke and Dr. Haisen Ta for technical instructions and providing the gold nanoparticle and intermediate filament samples; and Dr. Andreas Schönle for helping with Imspector. PX thank Prof. Stefan W. Hell for mentoring and training on STED nanoscopy instrumentation.

Author Contributions

Conceived and designed the experiments: PX QR DJ JAP. Performed the experiments: YL YD EA WZ. Analyzed the data: YL PX. Contributed reagents/materials/analysis tools: EA PJS WZ JT. Wrote the paper: YL PJS DJ PX.

References

  1. 1. Westphal V, Rizzoli SO, Lauterbach MA, Kamin D, Jahn R, et al. (2008) Video-rate far-field optical nanoscopy dissects synaptic vesicle movement. Science 320: 246–249.V. WestphalSO RizzoliMA LauterbachD. KaminR. Jahn2008Video-rate far-field optical nanoscopy dissects synaptic vesicle movement.Science320246249
  2. 2. Willig KI, Rizzoli SO, Westphal V, Jahn R, Hell SW (2006) STED microscopy reveals that synaptotagmin remains clustered after synaptic vesicle exocytosis. Nature 440: 935–939.KI WilligSO RizzoliV. WestphalR. JahnSW Hell2006STED microscopy reveals that synaptotagmin remains clustered after synaptic vesicle exocytosis.Nature440935939
  3. 3. Hofmann M, Eggeling C, Jakobs S, Hell SW (2005) Breaking the diffraction barrier in fluorescence microscopy at low light intensities by using reversibly photoswitchable proteins. P Natl Acad Sci U S A 102: 17565–17569.M. HofmannC. EggelingS. JakobsSW Hell2005Breaking the diffraction barrier in fluorescence microscopy at low light intensities by using reversibly photoswitchable proteins.P Natl Acad Sci U S A1021756517569
  4. 4. Hirvonen LM, Smith TA (2011) Imaging on the Nanoscale: Super-Resolution Fluorescence Microscopy. Aust J Chem 64: 41–45.LM HirvonenTA Smith2011Imaging on the Nanoscale: Super-Resolution Fluorescence Microscopy.Aust J Chem644145
  5. 5. Cao Y, Gan Z, Jia B, Evans RA, Gu M (2011) High-photosensitive resin for super-resolution direct-laser-writing based on photoinhibited polymerization. Opt Express 19: 19486–19494.Y. CaoZ. GanB. JiaRA EvansM. Gu2011High-photosensitive resin for super-resolution direct-laser-writing based on photoinhibited polymerization.Opt Express191948619494
  6. 6. Hell SW (2010) Far-field optical nanoscopy. In: Gräslund A, Rigler R, J W, editors. pp. 365–398.SW Hell2010Far-field optical nanoscopy.A. GräslundR. RiglerW. J365398editors.Single Molecule Spectroscopy in Chemistry, Physics and Biology: Springer. Single Molecule Spectroscopy in Chemistry, Physics and Biology: Springer.
  7. 7. Hell SW, Wichmann J (1994) Breaking the diffraction resolution limit by stimulated emission: stimulated-emission-depletion fluorescence microscopy. Opt Lett 19: 780–782.SW HellJ. Wichmann1994Breaking the diffraction resolution limit by stimulated emission: stimulated-emission-depletion fluorescence microscopy.Opt Lett19780782
  8. 8. Williamson DJ, Owen DM, Rossy J, Magenau A, Wehrmann M, et al. (2011) Pre-existing clusters of the adaptor Lat do not participate in early T cell signaling events. Nat Immunol 12: 655–662.DJ WilliamsonDM OwenJ. RossyA. MagenauM. Wehrmann2011Pre-existing clusters of the adaptor Lat do not participate in early T cell signaling events.Nat Immunol12655662
  9. 9. Hanssen E, Carlton P, Deed S, Klonis N, Sedat J, et al. (2010) Whole cell imaging reveals novel modular features of the exomembrane system of the malaria parasite, Plasmodium falciparum. Int J Parasitol 40: 123–134.E. HanssenP. CarltonS. DeedN. KlonisJ. Sedat2010Whole cell imaging reveals novel modular features of the exomembrane system of the malaria parasite, Plasmodium falciparum.Int J Parasitol40123134
  10. 10. Riglar DT, Richard D, Wilson DW, Boyle MJ, Dekiwadia C, et al. (2011) Super-resolution dissection of coordinated events during malaria parasite invasion of the human erythrocyte. Cell Host Microbe 9: 9–20.DT RiglarD. RichardDW WilsonMJ BoyleC. Dekiwadia2011Super-resolution dissection of coordinated events during malaria parasite invasion of the human erythrocyte.Cell Host Microbe9920
  11. 11. Rust MJ, Bates M, Zhuang X (2006) Sub-diffraction-limit imaging by stochastic optical reconstruction microscopy (STORM). Nat Methods 3: 793–796.MJ RustM. BatesX. Zhuang2006Sub-diffraction-limit imaging by stochastic optical reconstruction microscopy (STORM).Nat Methods3793796
  12. 12. Huang B, Wang W, Bates M, Zhuang X (2008) Three-dimensional super-resolution imaging by stochastic optical reconstruction microscopy. Science 319: 810.B. HuangW. WangM. BatesX. Zhuang2008Three-dimensional super-resolution imaging by stochastic optical reconstruction microscopy.Science319810
  13. 13. Shroff H, Galbraith CG, Galbraith JA, Betzig E (2008) Live-cell photoactivated localization microscopy of nanoscale adhesion dynamics. Nat Methods 5: 417–423.H. ShroffCG GalbraithJA GalbraithE. Betzig2008Live-cell photoactivated localization microscopy of nanoscale adhesion dynamics.Nat Methods5417423
  14. 14. Westphal V, Blanca C, Dyba M, Kastrup L, Hell S (2003) Laser-diode-stimulated emission depletion microscopy. Appl Phys Lett 82: 3125.V. WestphalC. BlancaM. DybaL. KastrupS. Hell2003Laser-diode-stimulated emission depletion microscopy.Appl Phys Lett823125
  15. 15. Rankin BR, Hell SW (2009) STED microscopy with a MHz pulsed stimulated-Raman-scattering source. Opt Express 17: 15679–15684.BR RankinSW Hell2009STED microscopy with a MHz pulsed stimulated-Raman-scattering source.Opt Express171567915684
  16. 16. Bückers J, Wildanger D, Vicidomini G, Kastrup L, Hell SW (2011) Simultaneous multi-lifetime multi-color STED imaging for colocalization analyses. Opt Express 19: 3130–3143.J. BückersD. WildangerG. VicidominiL. KastrupSW Hell2011Simultaneous multi-lifetime multi-color STED imaging for colocalization analyses.Opt Express1931303143
  17. 17. Moneron G, Hell SW (2009) Two-photon excitation STED microscopy. Opt Express 17: 14567–14573.G. MoneronSW Hell2009Two-photon excitation STED microscopy.Opt Express171456714573
  18. 18. Schrof S, Staudt T, Rittweger E, Wittenmayer N, Dresbach T, et al. (2011) STED nanoscopy with mass-produced laser diodes. Opt Express 19: 8066–8072.S. SchrofT. StaudtE. RittwegerN. WittenmayerT. Dresbach2011STED nanoscopy with mass-produced laser diodes.Opt Express1980668072
  19. 19. Wildanger D, Rittweger E, Kastrup L, Hell SW (2008) STED microscopy with a supercontinuum laser source. Opt Express 16: 9614–9621.D. WildangerE. RittwegerL. KastrupSW Hell2008STED microscopy with a supercontinuum laser source.Opt Express1696149621
  20. 20. Scheul T, D'Amico C, Wang I, Vial JC (2011) Two-photon excitation and stimulated emission depletion by a single wavelength. Opt Express 19: 18036–18048.T. ScheulC. D'AmicoI. WangJC Vial2011Two-photon excitation and stimulated emission depletion by a single wavelength.Opt Express191803618048
  21. 21. Willig KI, Harke B, Medda R, Hell SW (2007) STED microscopy with continuous wave beams. Nat Methods 4: 915–918.KI WilligB. HarkeR. MeddaSW Hell2007STED microscopy with continuous wave beams.Nat Methods4915918
  22. 22. Moneron G, Medda R, Hein B, Giske A, Westphal V, et al. (2010) Fast STED microscopy with continuous wave fiber lasers. Opt Express 18: 1302–1309.G. MoneronR. MeddaB. HeinA. GiskeV. Westphal2010Fast STED microscopy with continuous wave fiber lasers.Opt Express1813021309
  23. 23. Ding JB, Takasaki KT, Sabatini BL (2009) Supraresolution imaging in brain slices using stimulated-emission depletion two-photon laser scanning microscopy. Neuron 63: 429–437.JB DingKT TakasakiBL Sabatini2009Supraresolution imaging in brain slices using stimulated-emission depletion two-photon laser scanning microscopy.Neuron63429437
  24. 24. Bianchini P, Harke B, Galiani S, Vicidomini G, Diaspro A (2012) Single-wavelength two-photon excitation-stimulated emission depletion (SW2PE-STED) superresolution imaging. P Natl Acad U S A 109: 6390–6393.P. BianchiniB. HarkeS. GalianiG. VicidominiA. Diaspro2012Single-wavelength two-photon excitation-stimulated emission depletion (SW2PE-STED) superresolution imaging.P Natl Acad U S A10963906393
  25. 25. So PTC, Dong CY, Masters BR, Berland KM (2000) Two-photon excitation fluorescence microscopy. Annu RevBiomed Eng 2: 399–429.PTC SoCY DongBR MastersKM Berland2000Two-photon excitation fluorescence microscopy.Annu RevBiomed Eng2399429
  26. 26. Diaspro A, Chirico G, Collini M (2005) Two-photon fluorescence excitation and related techniques in biological microscopy. Q Rev Biophys 38: 97–166.A. DiasproG. ChiricoM. Collini2005Two-photon fluorescence excitation and related techniques in biological microscopy.Q Rev Biophys3897166
  27. 27. Xi P, Andegeko Y, Weisel LR, Lozovoy VV, Dantus M (2008) Greater signal, increased depth, and less photobleaching in two-photon microscopy with 10 fs pulses. Opt Commun 281: 1841–1849.P. XiY. AndegekoLR WeiselVV LozovoyM. Dantus2008Greater signal, increased depth, and less photobleaching in two-photon microscopy with 10 fs pulses.Opt Commun28118411849
  28. 28. Xi P, Andegeko Y, Pestov D, Lovozoy VV, Dantus M (2009) Two-photon imaging using adaptive phase compensated ultrashort laser pulses. J Biomed Opt 14: 014002.P. XiY. AndegekoD. PestovVV LovozoyM. Dantus2009Two-photon imaging using adaptive phase compensated ultrashort laser pulses.J Biomed Opt14014002
  29. 29. Wang W, Liu Y, Xi P, Ren Q (2010) Origin and effect of high-order dispersion in ultrashort pulse multiphoton microscopy in the 10 fs regime. Appl Opt 49: 6703–6709.W. WangY. LiuP. XiQ. Ren2010Origin and effect of high-order dispersion in ultrashort pulse multiphoton microscopy in the 10 fs regime.Appl Opt4967036709
  30. 30. Keller J, Sch nle A, Hell SW (2007) Efficient fluorescence inhibition patterns for RESOLFT microscopy. Opt Express 15: 3361¨C3371. J. KellerA. Sch nleSW Hell2007Efficient fluorescence inhibition patterns for RESOLFT microscopy.Opt Express 15: 3361¨C3371
  31. 31. Harke B, Keller J, Ullal CK, Westphal V, Schönle A, et al. (2008) Resolution scaling in STED microscopy. Opt Express 16: 4154–4162.B. HarkeJ. KellerCK UllalV. WestphalA. Schönle2008Resolution scaling in STED microscopy.Opt Express1641544162
  32. 32. Oliva A, Schyns PG (1997) Coarse blobs or fine edges? Evidence that information diagnosticity changes the perception of complex visual stimuli. Cognitive Psychol 34: 72–107.A. OlivaPG Schyns1997Coarse blobs or fine edges? Evidence that information diagnosticity changes the perception of complex visual stimuli.Cognitive Psychol3472107
  33. 33. Hyeon C, Dima RI, Thirumalai D (2006) Size, shape, and flexibility of RNA structures. J Chem Phys 125: 194905.C. HyeonRI DimaD. Thirumalai2006Size, shape, and flexibility of RNA structures.J Chem Phys125194905
  34. 34. Santangelo PJ, Lifland AW, Curt P, Sasaki Y, Bassell GJ, et al. (2009) Single molecule–sensitive probes for imaging RNA in live cells. Nat Methods 6: 347–349.PJ SantangeloAW LiflandP. CurtY. SasakiGJ Bassell2009Single molecule–sensitive probes for imaging RNA in live cells.Nat Methods6347349
  35. 35. Kasper R, Harke B, Forthmann C, Tinnefeld P, Hell SW, et al. (2010) Single-Molecule STED Microscopy with Photostable Organic Fluorophores. Small 6: 1379–1384.R. KasperB. HarkeC. ForthmannP. TinnefeldSW Hell2010Single-Molecule STED Microscopy with Photostable Organic Fluorophores.Small613791384
  36. 36. Huang B, Jones SA, Brandenburg B, Zhuang X (2008) Whole-cell 3D STORM reveals interactions between cellular structures with nanometer-scale resolution. Nat Methods 5: 1047–1052.B. HuangSA JonesB. BrandenburgX. Zhuang2008Whole-cell 3D STORM reveals interactions between cellular structures with nanometer-scale resolution.Nat Methods510471052
  37. 37. Vogelsang J, Kasper R, Steinhauer C, Person B, Heilemann M, et al. (2008) A reducing and oxidizing system minimizes photobleaching and blinking of fluorescent dyes. Angew Chem Int Edit 47: 5465–5469.J. VogelsangR. KasperC. SteinhauerB. PersonM. Heilemann2008A reducing and oxidizing system minimizes photobleaching and blinking of fluorescent dyes.Angew Chem Int Edit4754655469
  38. 38. Wurm CA, Neumann D, Schmidt R, Egner A, Jakobs S (2010) Sample preparation for STED microscopy. In: Papkovsky DB, editor. pp. 185–199.CA WurmD. NeumannR. SchmidtA. EgnerS. Jakobs2010Sample preparation for STED microscopy.DB Papkovsky185199editor.Live Cell Imaging, Methods in Molecular Biology.Totowa, NJ: Humana Press. Totowa, NJ: Humana Press.