In vivo optical imaging instruments have become mainstream tools for the visualization of molecular function and disease diagnostics. Fluorescence molecular tomography (FMT) offers an advantage over other optical imaging techniques in its ability to accurately quantify fluorescent signal.12.–3 Defining the performance of fluorescence tomography imagers is of primary importance because it is the ability to quantify fluorescent concentration that will spur the development of new biological applications. In FMT technology, fluorescence provides contrast between targeted and nontargeted tissues noninvasively4 using noncontact detectors.56.–7 For a sample of given optical properties, the emitted intensity is dependent on the distance between the source and the fluorescent object8 and on the intensity of the excitation beam.910.–11 Tomographic information is obtained at multiple projections, and the variation in fluorescence intensity at each projection is used to extrapolate spatial information.1213.–14 FMT image reconstruction computes the concentration of a fluorophore and its volume, making some assumptions about its absorption and scattering coefficients,15,16 knowing the sample thickness,17 and experimentally measuring the normalized Born approximation18 to retrieve the position, shape, and concentration of a target fluorophore.19 A three-dimensional (3-D) image is generated by creating a weight matrix of the sample, where voxel intensity values are assigned iteratively.15,2021.–22 However, in biological research, measuring fluorescence is effectively performed in a semiquantitative manner, and it is necessary for the user to define an “application-tailored” signal-to-noise ratio (SNR) and choose fluorophores based on the properties of the imager. From the user’s perspective, fluorescence emission intensity depends on the following variables: excitation intensity,23 spectral characteristics of the target fluorophore,2,24 spectral properties of the tissue sampled,25 and bandpass filters used; and it is ultimately proportional to fluorophore concentration. It follows that if the variable parameters can be controlled, emission can be measured consistently and the diffusion approximation11,22 solved for fluorophore concentration. As the major absorber of visible light in living organisms, hemoglobin plays a crucial role in light transmission and imaging gene activity effectively in vivo, beyond 600 nm is highly desirable; however, the number of applications using NIR fluorescent proteins is still small. The need to evaluate true in vivo performance of fluorescent proteins (FPs) within the visible spectral window is thereby crucial, given that the choice of unsuitable reporter fluorophores could lead to inaccurate results independent of FMT imager performance.
Here, the capabilities and limitations of a custom-built noncontact FMT system in localizing and quantifying fluorescent signal under variable experimental conditions were evaluated in vitro, in cell culture, and in vivo. To this purpose, we made use of a Tet-ON conditional gene expression system26 where five FPs were cloned in stable cell lines within the same genetic locus, thus resulting in identical mRNA expression levels. Since promoter activity was equal, it follows that variability in fluorescence emission intensity could be directly related to the activity of each FP (including brightness, stability, cell toxicity, and so on). In vivo validation of the FMT detection sensitivity was tested by targeting subcutaneous and deep-seated lymph nodes (LNs) in a transgenic mouse model. The FMT was used to quantify the T-cell population,27 focusing on how to overcome the practical challenges of detecting fluorescence from different anatomical locations. These data provide essential information for application design by establishing the quantitative accuracy, standardization, and reproducibility of the FMT imager. A calibration method was further established that enabled conversion of FMT signal intensity to molarity. In conclusion, these data describe a set of methodological steps that validate noncontact free-space fluorescence tomography in vitro and in vivo as an accurate technique for the detection and quantitative comparison of spectrally distinct fluorophores emitting between 520 and 660 nm.
Materials and Methods
The experimental noncontact FMT setup used [Fig. 1(a)] employed a continuous-wave argon-ion laser source (LaserPhysics, Reliant 1000m, West Jordan, Utah) emitting at 457, 488, and 514 nm and enclosed in a custom-built aluminum chamber coated in antireflective black coating (deep black optical paint, Gerd Neumann, Hamburg, Germany). The source was directed across three fixed mirrors (High Energy Argon-Ion Laser Mirrors, Edmund Optics, Barrington, Illinois) and a UV–NIR neutral density filter (Edmund Optics) into the FMT chamber and onto an optical scanner employing galvo-mirrors (Scanlab, SCANcube 7, Munich, Germany). Incident light power was measured before entering the optical scanner using a laser power meter (PH100-Si-OD2, Gentec Electro-Optics). The setup was designed to operate in both transmission and reflection geometries by repositioning a mirror (First Surface mirror, Edmund Optics) mounted on a travel linear translation stage (Edmund Optics). The sample holder was mounted on an electronically controlled positioning stage (Standa, Vilnius, Lithuania). A custom-built filter wheel accommodating up to five filters was aligned to a 50 mm Macro objective (SIGMA Corporation, Tokyo, Japan). Light collection was performed using a -, -, -, or interference bandpass filters (Andover Corporation, Salem, New Hampshire) to isolate fluorescence from excitation light. A 16-bit, charge-coupled device (CCD) (DV 434, Andor Technology, Belfast, Northern Ireland), thermoelectrically cooled down to , was used for the detection of signals. The lens was focused on the surface of the sample, and the image scaled from pixel dimensions to metric units by the use of metric fiducials. Stage calibration was performed to convert the CCD field of view to degrees of rotation of the galvo-mirrors. For all experiments, an image was obtained with white light illumination before exposure to the laser source and was used as a reference image for source pattern selection. Additionally, a background image in the absence of an illuminating source was acquired to account for any external light entering the FMT chamber. Illumination sources were distributed symmetrically to the target location for both reproducibility and calibration experiments. Exposure time used was 0.2 s with 0.8 mW excitation power. Identical source/detector parameters were used for the fluorophores Atto590 (excitation max 594 nm, emission max 624 nm; ATTO-TEC Gmbh, Germany) and carboxyfluorescein succidimyl ester (CFSE) (excitation max 492 nm, emission max 517 nm; Thermo Fisher Scientific Inc.) placed in a 2-mm capillary glass tube in a phantom at a depth of 3 mm from the surface. A slab geometry phantom was used with a combination of 20 ppm India ink and 1% Intralipid-20% to match tissue-like optical properties at 520 nm (scattering coefficient and absorption coefficient ) and at a depth of 12 mm. An isoflurane vaporizer was used to deliver anesthetic to the FMT chamber and to the induction chamber, and a scavenging system was used to remove excess anesthetic gas (Fluovac systems, Harvard Apparatus, Hollison, Massachusetts).
Tomographic Data Acquisition and Reconstruction
Tomographic imaging was performed by scanning the laser source into selected illumination points.23 The optimum excitation source pattern found for the tomographic scans was an grid covering a field of view of . For each illumination point, two measurements (excitation and emission) were recorded sequentially with the appropriate bandpass filters placed in front of the CCD. An image stack was created for all illumination points creating two sets of raw data (excitation and emission). Excitation and emission stacks were then resampled to a detector grid covering the target area and used for the tomographic reconstructions. Data from the excitation and emission stacks were used to create the normalized Born ratio18 as shown in the following equation:Figs. 1(b)–1(e)] was performed using diffusion theory and modeling light propagation16 in free space5 in a homogenous slab solution.8,19 The tissue medium below the detector area was discretized to a total of 2700 voxels of centered to the target area. Data inversion was performed using an iterative approach,20,21,28 and 3-D reconstructions were obtained with 100 iterations (Table 1). For phantom experiments, a cylindrical region of interest (ROI) was selected and the mean intensity value was used for quantification. Variation of the number of iterations did not affect the ROI mean. The source/detector patterns used in transmission geometry were identical to those in reflection modality (10 mW excitation power and 2 s exposure time). Data acquisition and processing were performed on a 3.0 GHz Pentium D with 512 MB RAM, and the system was controlled by custom-built software using LabView (National Instruments, Austin, Texas) system design software.
Comparative statistical analysis for quantification experiments in reflection (R) and transmission (T) modalities. Phantoms with increasing concentrations of CFSE and Atto590 were imaged with the FMT and emission quantified for each dataset. The correlation between the linear regression model used and the experimental data points is illustrated by the R2 and SDM values. The slope values were used as means to compare reproducibility between modalities. Increasing the number of iterations from 100 to 1000 marginally improves the fits (bold) and the slope. Small differences in slope values can be noticed between reflection and transmission experiments, indicating that a quantitative comparison of values between modalities is possible but may be affected by the intensity range.
Fluorescence Molecular Tomography Calibration
Fluorophore quantum yield (QY) defines the efficiency with which absorbed light is converted to emitted light. Published QYs, however, are recorded at excitation and emission maxima. Such conditions often fail to match experimental conditions due to the wavelengths available and also because experimentally the QY is affected by concentration range and solvent properties. Commercial QY values therefore could not be used for FMT imaging calibration; we used the linear quantification data from CFSE and Atto590 to calculate the FMT-fluorescence yield (FMT-FY) described for our samples and experimental parameters. A plot of FMT-recorded intensities () (-axis) against measured sample absorbance (-axis) (FluoroMax, Jobin Yvon, Horiba Scientific, Kyoto, Japan) was obtained by multiplying the known fluorophore concentrations () by their published extinction coefficient values () and measured light path length () following Beer–Lambert’s law:
The absorbance values were then plotted and fitted to a linear regression model, as shown in Fig. 2. The slope of the fits () is proportional to the QY of the fluorophore, where is the intercept on the -axis:
FMT-FY values were calculated using a standard (st) solution as reference; is thus always expressed as relative to as follows:
The calculated FMT-FY for CFSE and Atto590 was
The ratio of the calculated FMT-FYs () was then compared with the ratio between the slopes ():
The calculated slopes were proportional to the FMT-FYs and consequently to the fluorophores’ QYs (within 10% error). The linear relationship between fluorescence emission intensity and concentration [Eq. (4)] therefore becomes:Table 2.
Conversion table. The molar concentrations of CFSE and Atto590 used and the intensity values (a.u.) recovered from the 3D-FMT data analysis are shown. FMT concentration values represent the converted a.u. units to molarity obtained by the FMT calibration step.
|FMT intensity||FMT concentration|
|CFSE concentration (μM)|
|Atto590 concentration (μM)|
Stable HeLa cell lines expressing enhanced yellow fluorescent protein (EYFP), super green fluorescent protein (SGFP), enhanced green fluorescent protein (EGFP), Katushka,29 or Cardinal30 red fluorescent protein were generated and characterized as described by Weidenfeld et al.26 In brief, HeLa Tet-ON advanced cells (line EM2-11ht) were stably transfected with DNA coding for the fluorescent proteins under control of a tetracycline/doxycycline inducible promoter (Ptet). The gene of interest was stably integrated into a defined genomic locus (5q31), which allows tight regulation of the doxycycline-inducible expression. Constructs were inserted by Flippase Recombinase-Mediated Cassette Exchange (Flp-RMCE), and clonal lines were isolated. The expression characteristics of the derived cell lines were directly comparable as the transgenes were directionally integrated as single copies at the same locus. HeLa cells were cultured in DMEM supplemented with 10% FBS, 2 mM glutamine, and 1% penicillin/streptomycin. Expression of SGFP, EGFP, EYFP, Katushka, or Cardinal was induced by doxycycline, supplied to the media at . For FMT imaging of HeLa monolayers, 24-well tissue culture plates were used.
Rag1−/−,31,32 CD2,33 and DsRed34 transgenic animals were maintained in the Institute of Molecular Biology and Biotechnology colony. For the FMT imaging, the animals () were anesthetized with 1.5% isoflurane, initially delivered at 2.5% in a tranquilizing chamber. Temperature and breathing of each animal were monitored during the experimental procedure. Mesenteric nodes (MNs) were detected after feeding the mice for 2 weeks with alfalfa-free food (Labdiet), and hair was removed using depilatory cream. All animal experimental protocols were conducted in accordance with and under the approval of the Foundation for Research and Technology Ethics Committee and the General Directorate of Veterinary Services, Region Crete (permit numbers: EL 91BIO-02 and EL91-BIOexp-02).
Cell Culture Experimental Protocol
A 24-well cell culture plate containing HeLa-wt and stable HeLa clones expressing either EGFP, EYFP, SGFP, Katushka, or Cardinal () was imaged using a two-dimensional (2-D) raster scan, ensuring homogeneous excitation across samples. The EGFP-, SGFP-, and EYFP-positive cells were excited using the 488-nm laser line, and emission was recorded with -nm and a filters. Katushka- and Cardinal-positive cells were excited with the 514-nm laser line, and -nm and filters were used for emission. SGFP-positive cells were measured with all filter sets. To mimic the high absorbance, freshly heparinated mouse blood was added to the culture wells to a final concentration of 12% (assuming a molar extinction coefficient of 24202.4  at 520 nm, matching ). ROI areas (identical for all samples) corresponding to the width of the wells were used to quantify FP emission. The data were normalized for filter width, excitation, and emission wavelength and for cell number. Fluorimeter data were experimentally measured for each population at .
In Vivo Experimental Protocol
Initially, a 2-D scan was performed on each animal to locate the target LN using 514-nm excitation and emission (1 mW excitation power and 6 s exposure time). These images were used to determine the scan pattern position: a source grid was chosen to cover a wide field of view () with 25 mW excitation power and 0.2- to 0.6-s exposure time for the superficial and deep targets, respectively. Tomographic data were recorded using 514-nm excitation with -nm and a emission filters for fluorescence measurement and a filter to measure the excitation field. The data were processed with in-house developed software using a detector pattern.
In Vitro Quantification
In order to assess the capabilities of the FMT system, a set of experiments was designed to address its sensitivity, dynamic range, and resolution. Each query was dependent on the SNR and was therefore application dependent. Given that the optical properties of the fluorescent object of interest and its immediate surroundings significantly affected the SNR, each experiment here reported was acquired using settings where the SNR was experimentally maximized. A typical 3-D-reconstructed image is shown in Fig. 1. The FMT imager was tested in reflection and transmission geometry modes at different wavelengths. Initially, response was assessed with phantoms containing 2, 4, 8, and of CFSE in reflection geometry. To compare the quantification accuracy at different spectral regions, CFSE was replaced with Atto590. Atto590 has a high molecular absorption and a high QY (0.80); however, the 514-nm source achieved approximately 10% excitation efficiency. This resulted in a 60% weaker Atto590 emission compared with CFSE (excitation max 489 nm). Atto590 concentrations (5, 10, 15, and ) were chosen to match the intensity range used for CFSE. Similarly, a set of experiments assessed the quantification capabilities of the FMT imager in transmission geometry. Quantification of mean intensity values in transmission geometry was achieved using the same reconstruction and ROI parameters used for reflection and were therefore directly comparable. The results from the quantification analysis for CFSE and Atto590 in reflection and transmission modes (Fig. 3) were fitted to a linear regression model (Table 1). The quantification data showed the reconstructed fluorescence mean intensity values to be linearly proportional to fluorescence concentration.
In Vitro Reproducibility
The FMT imager’s reproducibility was then assessed by designing a set of in vitro experiments carried out in reflection geometry using CFSE. Data acquisition, processing, ROI selection, and quantification were obtained (excitation 488 nm, emission ; source/detector pattern, 100 iterations) for four independent measurements performed as technical repeats. Reproducibility was assessed by standard deviation of the mean (SDM) and standard error of the mean (SEM), and , respectively, 2 and 3 orders of magnitude smaller than the mean (0.00204 a.u.), with a coefficient of variance of 0.00792 indicating a systemic error . Conversion using the calibration factor in Eq. (4) recovered a value of .
Optimal Fluorescent Protein Selection for Fluorescence Molecular Tomography
The intrinsic properties of fluorescent proteins dictate whether or not they are suitable for an application; however, these are seldom explicitly tested. The relative intensities of the emission displayed by identical numbers of HeLa cells expressing YFP, SGFP, EGFP, Katushka, or Cardinal were obtained by quantifying the mean FMT reconstructed values. The mean intensity values recorded [Figs. 4(a) and 4(b)] were corrected for filter width. These normalized data give a more accurate intensity value for each fluorophore considered; more precisely, they represent a weighted average across the filter wavelength range.
For increased spectral resolution, a dedicated spectral imager2 would be required. Green emitters were approximately 1 order of magnitude brighter than red emitters. The data were further corrected for the “excitation efficiency” term achieved by the available laser lines (488 and 515 nm). To address the nonlinear relationship between excitation wavelength and emission intensity, the values were corrected by an experimentally defined “efficiency factor” as follows:
, , and intensity values were obtained using a fluorimeter, where spectral data were measured using each cell line. Figure 4 shows how, even by exciting at the excitation peak, red emitters still display weak emission and GFP emission is still clearly detectable using a filter. The data were then corrected for the “emission efficiency” achieved: the emission spectral profiles obtained for the cells were used to calculate the integrals for the whole emission curve and, separately, the integrals for the wavelengths covered by each filter used to image the sample with the FMT as follows:
• 510-nm filter: 505 nm → 515 nm;
• 540-nm filter: 520 nm → 560 nm;
• 593-nm filter: 573 nm → 613 nm; and
• 615-nm filter: 570 nm → 660 nm.
The ratio of the “whole emission curve”/“detected emission” represents the portion of fluorescent signal actually detected by the FMT:
The “corrected” values [Figs. 4(c) and 4(d), dashed lines] represent the achievable values by exciting the fluorophores at their excitation maximum and detecting the whole of the emission curve. A final correction that could be made to these values is defined by the QY. This correction should, in theory, equalize the values for the different fluorophores at identical concentrations. Unfortunately, QY information for the specific fluorescent proteins used here was unavailable at the time of writing.
In Vivo Small Animal Imaging
LNs represent highly desirable targets for in vivo imaging due to their functional importance to the immune system. An immune response is in fact a localized process with LNs acting synergistically while remaining independent from one another. To test whether the FMT could resolve fluorescence from anatomically diverse LNs, the inguinal and mesenteric LNs of a CD2/DsRed mouse were targeted. The inguinal LN is located subcutaneously at the height of the groin, while the MNs are found bunched (usually five to six nodes) deep within the mesentery of the intestine. Figure 5 shows the raw fluorescence data (a) and the 3-D reconstructed image (b) for the right inguinal LN of a CD2/DsRed mouse. The FMT software correctly located the origin of the fluorescent signal, and the reconstructed image matched the dimensions and anatomical conformation of the inguinal LN. The mesenteric LNs of a CD2/DsRed and a nonfluorescent control mouse were then targeted (Fig. 6). The morphology and location of the MNs make target recognition a difficult task; however, the DsRed-positive reconstructed image displayed three times as much fluorescent signal than the control sample. The bright autofluorescent object visible in both the control and DsRed animals was identified ex vivo as the gallbladder. The DsRed signal located at 0.5 to 1 cm below the gallbladder is consistent with the MNs.
The performance of a noncontact FMT system was demonstrated by assessing its quantification accuracy and data reproducibility within 520- to 660-nm windows of the visible spectrum. These data reflect biologically valuable wavelengths, given that most fluorescent proteins and dyes in current use emit light within that range. These wavelengths are particularly challenging for quantitative optical imaging setups, given that the contribution of autofluorescence, scattering, and absorption by biological tissues is nonlinear. It is useful to note that although NIR fluorescent proteins and probes have been developed over the past decade, their use in biological applications is still lagging compared with well-established green fluorescent proteins such as GFP, and the use of many markers, including fluorescently labeled antibodies, used in fluorescence microscopy has not been widely translated to an in vivo setting. The nonlinear attenuation of light transmission in turn affects the ability to compare fluorescence emissions from different anatomical regions. In practice, this means that, in a typical experimental design, fluorophores are compared with a control sample group (e.g., before and after a treatment) and only rarely to a spectrally distinct fluorophore. It is therefore important to establish a method that enables the quantitative detection of fluorescence, regardless of anatomical location and wavelength. Reconstructed FMT intensities were here found to be linearly dependent on fluorophore concentration, and this result was reproduced irrespective of wavelength and acquisition geometry, strengthening the notion that FMT can accurately retrieve concentration values for subsurface and deeper-seated ROIs. The reproducibility of the FMT data was evaluated by three parameters: (1) the SNR was optimized experimentally to reduce variance between background and target-specific emissions; (2) SDM between FMT intensity and fluorophore concentration was used as an indicator of dynamic range; and (3) SDM of repeated measurements was used as an indicator of technical accuracy. Standard deviation and standard error values throughout this study were consistently found to be at least 1 to 2 orders of magnitude smaller than the mean intensity value across intensities. A protocol for the calibration of the FMT system was established that allowed converting FMT intensity values to fluorophore concentrations, with accuracy values that reflected experimental variability. Repeated measurements were performed, and the variance between measurements was found to be to . FMT quantification accuracy within the visible spectrum was therefore in the nanomolar range and formalized by the variance coefficient at . The relative strength of five fluorophores was evaluated in the presence of blood in order to mimic the most challenging in vivo settings. The absorption properties of the heme group around 500 nm significantly affected the excitation light penetration. During data processing, the normalization of excitation and emission light resulted in an apparent increase of fluorescence in the presence of blood, dictated by a difference in absorbed excitation light. It is clear from these data that FP performance should be experimentally validated for each application and imaging setup characteristic. Most red emitters were found to be approximately 1 order of magnitude less bright than EGFP and EYFP; therefore, in cases where excitation/emission excitation was suboptimal, red FPs could be outperformed by green FPs. The translational potential of these results to an in vivo setting was demonstrated here by the detection and reconstruction of fluorescently labeled T-cells in vivo. The FMT imager correctly located two spectrally and anatomically distinct regions: the inguinal LNs and the MNs of a transgenic CD2/DsRed mouse. The quantification accuracy of the fluorescent reconstructions in vivo was assessed separately using flow cytometry data.27 Cumulatively, the data demonstrate that noncontact FMT can perform quantitative fluorescence imaging in vitro and in vivo in a window of the visible spectrum with high precision and provide the advantage of quantitatively comparing fluorescent emissions across a wide spectral window, regardless of anatomical location.
This work was supported by the FP7 EU Grant “FMT-XCT.” RF acknowledges support from the Marie Curie Early Stage Training Grant “EST-MolecImag.”
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Rosy Favicchio, PhD, is a molecular biologist who specializes in the development of in vivo imaging technologies for the study of biological dynamics with a keen interest in metabolism. She is currently a research fellow at Imperial College London where she is developing theranostic tools applied to cancer research.
Stylianos Psycharakis is currently a PhD student at the University of Crete and a member of the In vivo Imaging Lab, Institute of Electronic Structure & Laser, Foundation for Research and Technology—Hellas, Heraklion Crete, Greece. His research interests include the design and realization of novel 3-D Micro-scopic imaging techniques such as Selective Plane Illumination Microscopy and Optical Projection Tomography and their application in studying dynamic biological processes.