Knowledge of the spatial distribution of lipids in the intraocular lens is important for understanding the physiology and biochemistry of this unique tissue and for gaining a better insight into the mechanisms underlying diseases of the lens. Following our previous study showing the spatial distribution of sphingolipids in the porcine lens, the current study used ultra performance liquid chromatography quadrupole time-of-flight mass spectrometry (UPLC-QTOFMS) to provide the whole lipidome of porcine lens and these studies were supplemented by matrix-assisted laser desorption ionization mass spectrometry imaging (MALDI MSI) of the lens using ultra-high resolution Fourier transform ion cyclotron resonance mass spectrometry (FTICR MS) to determine the spatial distribution of glycerophospholipids. Altogether 172 lipid species were identified with high confidence and their concentration was determined. Sphingomyelins, phosphatidylcholines, and phosphatidylethanolamines were the most abundant lipid classes. We then determined the spatial and concentration-dependent distributions of 20 phosphatidylcholines, 6 phosphatidylethanolamines, and 4 phosphatidic acids. Based on the planar molecular images of the lipids, we report the organization of fiber cell membranes within the ocular lens and suggest roles for these lipids in normal and diseased lenses.
Citation: Pól J, Vidová V, Hyötyläinen T, Volný M, Novák P, Strohalm M, et al. (2011) Spatial Distribution of Glycerophospholipids in the Ocular Lens. PLoS ONE6(4): e19441. https://doi.org/10.1371/journal.pone.0019441
Editor: Valdur Saks, Université Joseph Fourier, France
Received: January 19, 2011; Accepted: March 29, 2011; Published: April 29, 2011
Copyright: © 2011 Pól et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This work was supported by funding from the Sigrid Juselius Foundation (JMH), The Finnish Eye Foundation (JMH), the Academy of Finland (JP project No. 122354), research funds from the University of Helsinki (SKW: University of Helsinki project No. 2105060), the Ministry of Education, Youth, and Sports of the Czech Republic (LC07017), the Institutional Research Concept of the Institute of Microbiology, and the Academy of Sciences of the Czech Republic (AV0Z50200510). MV is supported by a Marie Curie IR Grant within the EC FP7 and by the Czech Science Foundation (Project P206/10/P018). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
The ocular lens is a unique epithelial tissue responsible for fine-tuning images projected onto the retina. To present a sharp and clear image, the lens needs to be transparent, minimize light scattering, and must be able to change its curvature. The mammalian lens is composed of lens fiber cells derived from a single layer of lenticular epithelial cells. As the lens ages, the fiber cells elongate and the older cells are packed toward the center of the lens, forming concentric onion-like layers of fiber cells. The oldest cells are positioned in the innermost segment of the lens (nucleus), whereas the younger cells are located in the cortical region (cortex) of the lens. The lens fiber cells are precisely aligned with the adjacent cells and also contain high amounts of crystallins, specialized soluble proteins. These pzroteins give the fiber cells a significantly higher refractive index than the fluids around the lens and also reduce light scattering . Due to the loss of internal organelles from the fiber cells , the plasma membrane eventually becomes the only cellular organ of the lens. This membrane is unique in that it contains high concentrations of the integral membrane protein aquaporin 0 (AQP0), a 26 kDa water channel, and in that it lacks polyunsaturated phospholipids and contains high concentrations of sphingolipids and cholesterol –.
Mass spectrometry imaging (MSI) allows for the visualization of molecular maps through its automated raster-collection of mass spectra from a tissue surface . Several direct desorption ionization techniques have been developed to operate in MSI mode. Matrix-assisted laser desorption ionization (MALDI) , , desorption electrospray ionization (DESI) , and secondary ion mass spectrometry (SIMS)  are the most common techniques. As an emerging technology, MSI has already been targeted to address biological (mal)functions , , and this technique and its applications have been reviewed ,  and a protocol has been established . MSI benefits from its power to visualize spatial chemical distribution across a tissue. One of the limitations of MSI is problematic quantification. Desorption and ionization of a compound from a tissue during MALDI MSI is influenced by the MALDI matrix type, its thickness, size of crystals, and the quality of the tissue surface. Diverse anatomy of a tissue (accompanied by native chemical changes) is responsible for variations of MALDI signal response. The use of internal standard in MALDI MSI has not yet been established and therefore only relative quantitative changes of an ion signal can be measured. Accordingly, absolute concentrations cannot be obtained and thus it would be advisable to use other techniques allowing for quantitative assessment of the whole lipidome. Ocular lens is a tissue, which anatomy is simple and its nucleus and cortex forms quite uniform structure. Therefore we anticipate small variation in MALDI signal response across the tissue slice. Quantification of about 100 phospholipids in the whole human and animal intraocular lenses has been performed using ESI-MS . That study showed phosphatidylcholines (PCs) to be the most abundant lipids in porcine lens, followed by sphingomyelins (SMs), phosphatidylethanolamines (PEs), phosphatidylserines (PSs), and dihydro-SMs, respectively. A review describing lipid functions in ocular lens has recently been published .
The regional distributions of phospholipids in ocular lenses have been assessed using matrix assisted laser desorption ionization time-of-flight (MALDI-TOF) and 31P nuclear magnetic resonance (NMR) analyses of extracts of surgically separated concentric sections , . In those studies, the concentrations of phospholipids were the highest at the cortex of the lens and decreased toward the lens nucleus. The changes in the distribution of spatial phospholipids were assessed based on the compositional average from relatively large sections of the lens, and therefore the spatial resolution of the experiment was low and no detailed differences in lipid concentrations were observed. The in situ spatial analysis of the phospholipids of the lens by direct MALDI-TOF MS analysis was conducted by averaging mass spectra acquired from three or four spots next to each other from the cortex and the nucleus . Although these experiments provided the precise lipid composition at particular spots of the lens, the distribution of lipids in the context of the whole lens remained unclear. As was previously mentioned, several desorption-ionization techniques are available for mass spectrometry imaging and selecting the appropriate technique is crucial. Recently, the research group of Blanksby reported  the use of MALDI for mass spectrometric visualization of dihydrosphingomyelin (d18∶0/16∶0) and dihydroceramide (d18∶0/16∶0) in human lenses. Similarly, DESI has served for imaging of cholesterol, sphingomyelins, and glycerophospholipids .
We elucidated the spatial distribution of sphingolipids in the porcine lens using MALDI MSI and provided detailed information about compositional changes in the clear lens nucleus and cortex . Following our previous observations, we now provide the whole lipidome of clear porcine lens and also determine the spatial distribution of 30 glycerophospholipids (GPs) using a combination of ultra performance liquid chromatography quadrupole time-of-flight mass spectrometry (UPLC-QTOFMS) and MALDI imaging coupled to Fourier transform ion-cyclotron resonance mass spectrometry (FTICR MS). Although TOF MS is commonly used in MSI, FTICR MS is preferred due to its superior mass resolution and mass accuracy, which allows unambiguous peak recognition and precise assignment of exact masses. Thus, FTICR MS allows for the identification of molecular formulae with increased confidence.
Results and Discussion
To begin with, porcine lenses were extracted and analyzed with UPLC-QTOFMS to obtain global lipid profile of the whole lens. The identified lipids are listed in supplementary Table S1, and the most abundant lipid classes are shown in Figure 1. SMs, PCs and PEs were the most abundant identified lipids in the lens. Of these, the number of individual PC species was clearly the highest. The lipid profiles in different lens samples were very similar, the overall deviation of the amount of lipids was on average <30%. These results are in relatively good agreement with Deeley et al. . These authors found that PCs were the most abundant lipids, followed by SMs, PSs, and PEs. Overall, Deeley et al.  identified 71 lipid species (22 PEs, 16 PCs, 14 PSs, 13 SMs, 3 phosphatidylinositols, and 3 phosphatidic acids (PAs)). Of these lipids our analysis identified 50%. Most notably due to technical reasons negatively charged phospholipids (such as PSs, phosphatidylinositols, and PAs) were not found among our analysis. However, compared to the study of Deeley and coworkers we were able to identify and quantitate altogether 101 new lipids. Interestingly, 36 triglyceride species were also identified suggesting that some energy storage in epithelial cells has to remain.
Each bar represents the mean concentration of six lens extracts. Error bars are standard deviations of six individual measurements. The y-axis is given as nmoles/mg of lens protein. LysoPC, lyso-phosphatidylcholine; PC, phosphatidylcholine; PE, phosphatidylethanolamine; SM, Sphingomyelin; TG, triglyceride.
Following our previous study, in which we described the spatial distribution of SMs in porcine lens using MSI , we have now resolved the spatial distribution of 30 GPs in the same tissue including 20 PCs, 6 PEs, and 4 PAs (Table 1, Figure 2). It is obvious that a notable fraction of lipid species were not, however, identified in the MSI experiment in comparison to the UPLC-QTOFMS analysis of the whole lens extract. This is partly due to the small sampling area (50 µm) of the MALDI laser in imaging mode. Yet, as can be seen most of the high abundance lipids detected by UPLC-QTOFMS were identified also by MALDI MSI.
The lipid intensities were measured using matrix-assisted laser desorption ionization mass spectrometry imaging (MALDI MSI) of the lens using ultra-high resolution Fourier transform ion cyclotron resonance mass spectrometry (FTICR MS). Error bars represent standard deviation of 3 samples. Mean intensities can be equally (in relative scale) compared only within one lipid class.
Figure 3 displays averaged mass spectra in the mass range of all identified lipid species and also several zoomed parts. The enlargements demonstrate how important it is to use ultra high-resolution mass spectrometry for imaging. Analyte peaks are separated from peaks originating from the biological and MALDI matrices. The use of lower resolution instrumentation would result in overlapping of analyte peaks with the interferences. As a consequence, the spatial distribution of lipids can be compromised. In our experiment we observed interferences in proximity of glycerophosholipid peaks (shown only for sodium adducts) at the following nominal masses: 506, 697, 700, 723, 728, 754, 780, 806, 808, and 810 m/z.
In the top spectra, circle on a crest of mass peaks indicates sodium adducts of the identified glyceroposholipids. At the bottom, we demonstrate using nominal m/z 697, 700, 780, and 808 the importance of the use of high-resolution MS in imaging. Analyte peaks are separated from interfering biological and MALDI matrix peaks.
PCs composed the largest group by number of lipids identified by MALDI MSI in keeping with UPLC-QTOFMS and also in line with findings from other epithelia cells, in which PCs are the major lipid class. For PCs with 14–20 (lyso-forms) and 34–36 carbons in their acyl chains, the mean intensity of the lipids was higher in the cortex than in the nucleus. These findings are in accordance with the previous work of Rujoi et al. . In contrast, PCs with 20–32 carbons in their acyl chains had higher mean lipid intensities in the nucleus compared to the cortex. Markedly these lipids were saturated in contrast to all other diacyl lipids identified. The high concentration of saturated and long acyl chain lipids make the cellular membranes significantly more rigid in the nucleus compared to the fluid like membranes in the cortex. Also the higher concentration of rigid SMs  in the nucleus further rigidifies the plasma membrane. This finding may reflect the slow metabolism of the nuclear fiber cells. PCs were identified as protonated, sodium, and potassium adducts. It should be noted that comparison of mean intensities is only relevant within one lipid class (Figure 2), since ionization desorption efficacy differs from one lipid class to another.
The second most abundant group of lipids consisted of 6 PEs∶ lysoPE (16∶1), lysoPE (18∶0), and lysoPE (18∶1), which all were identified as sodium and potassium adducts, had a higher mean intensity in the cortex than in the nucleus. In contrast, PEs containing two acyl chains (PE(36∶3), PE(36∶4), and PE(38∶4)) had a slightly higher abundance in the nucleus compared to the cortex. The distribution of diacyl and unsaturated PEs was just the opposite compared to diacyl unsaturated PCs (Fig. 2).
Finally, 4 PAs were also identified and their spatial distribution resolved: a single lysoPA (18∶1), and diacyl PA (32∶1), PA (34∶1), and PA (36∶2). All lipids were identified as sodium and potassium adducts and two of these PAs ((PA (34∶1) and PA (36∶2)) were among those detected also by Deeley et al. . All PAs had a higher mean intensity in the nucleus compared to the cortex.
Figure 4 presents a typical image of the spatial distribution of PC (34∶2). The nucleus and the cortex are easily visualized through the changes in the spatial concentration of this PC as well as the fine structures of the lens, since the PC localizes to the equatorial margins where the germination zone resides. In the adult lens, almost none of the epithelial fiber cells are dividing. In the germinal zone, the lens epithelial cells proliferate slowly. This suggests that the newly formed cells contain high amounts of PCs with relatively high amounts of intracellular organelles. As the cells differentiate and the intracellular organelles are lost , the relative content of PC decreases.
The lens cortex is the area between the nucleus and lens borders. Equatorial margins are clearly defined by the high abundance of phospholipids, and the lens nucleus is less visible in this case due to the changes in lipid composition in the lens.
A trend in spatial distribution as a function of acyl chain length can be observed for all GPs analyzed (Figure 5). LysoGPs, except lysoPA, exhibit higher mean intensities in the cortex than in the nucleus (Figures 2 & 5), and they are distributed evenly across the whole cortex area. On the contrary, GPs with two saturated acyl chains have a higher mean intensity in the nucleus than in the cortex (except for PCs with acyl chains of 18 carbons, which have the same mean intensity in the nucleus and the cortex) and tend to localize to the equatorial margins. It is presently unknown how this concentration gradient is maintained. Degradation would decrease the lysolipid content toward the nucleus. It is quite unlikely that the lysolipids would be acylated as the lens matures. Alternatively, in the developing lens high amounts of lysolipids could act as surfactants and hamper the development of the lens cortex, whereas the mature lens may accommodate the lysolipids more easily.
MALDI-MS images were acquired by an APEX Ultra 9.4 T FT-ICR mass spectrometer equipped with a Smart beam laser. The molecular images of the lipids were visualized using the FlexImaging software, and the intensity of the image was normalized to the total ion chromatogram. Identification of lipids was performed from the average spectra of the entire lens using Mass data analysis software.
The spatial distribution of lipids described here correlates well with previous observations on the spatial distribution of the most abundant integral lens membrane protein . Full-length AQP0 was found throughout the lens, but its concentration increased toward the periphery of the lens. In contrast, the major truncation product of AQP0 (amino acids 1–246) was absent from the lens periphery but was present and increased in abundance closer to the nucleus. In keeping with previous ESI-MS experiment  our results suggest that SMs and PCs are the most abundant lipids in the porcine lens. PCs are almost universally the most abundant lipid species across different species as well as in various cell types and are believed to provide an optimal platform for the functioning of integral and soluble membrane proteins. In many cell types, PCs are also important sources of lipid second messengers, but in metabolically inactive tissues such as the lens, this property/function seems unlikely. The presence of saturated acyl chains increases toward the nucleus (see PC (28∶0) and PC (30∶0)). As we have previously shown, this trend occurs with all but one identified SM  and suggests that these lipids play a functional role in the lens nucleus by providing stiffer membranes that are more resistant to various stress factors. In contrast, the polyunsaturated PCs are found primarily in the cortical regions of the lens. PAs and PEs, which have a major effect on the lateral pressure profile of membranes , show a similar spatial distribution, whereas the relative concentrations of PAs and PEs are just the opposite; the concentration of PAs increases toward the nucleus, whereas PEs are found at higher concentrations in the cortex. These diffzerences may play a role in the regulation of whole length AQP0 and the truncation product of AQP0.
In conclusion, UPLC-QTOFMS unambiguously identified lipids from tissue samples through the determination of their molecular formulae by exact mass measurements. By FTICR ultra-high resolution mass spectrometry we were now able to provide the spatial lipid distribution of >20% of all lipids in the porcine lens. Since tandem mass spectrometry of lipids ionized directly from the tissue sample is not feasible for most of the identified lipids due to their low ion intensities, this method represents an elegant and reliable analytical approach. The spatial distribution of GPs provided by mass spectrometry imaging reveals the organization of lipid membranes in a healthy porcine ocular lens. These data along with the known spatial organization of membrane proteins supplements current knowledge of cell membrane functions. The long-term goal of our ongoing studies is to characterize the lipid distribution of clear and cataractous human lenses and thus provide mechanisms to understand diseases of the lens.
Materials and Methods
Basic Experimental Principle
We used MALDI MSI to investigate the spatial distribution of GPs in a porcine ocular lens. In MALDI MSI, compounds are ionized directly from the tissue slice, which is attached on a conductive surface moving in set raster steps under a laser beam. Mass spectra collected from each point within the raster are used to assemble the molecular images in correlation with their x- and y- positions. The tissue surface is uniformly coated by the deposition of a matrix aerosol to ensure co-crystallization with lipids, which facilitates desorption and ionization. The coating process is computer controlled to avoid excessive over-wetting, which would deteriorate the spatial distribution of the molecules in the tissue. Ions desorbed from the tissue are accelerated into the mass spectrometer for separation based on the mass-to-charge ratios of the ions and detected. Sampling of the ions directly from the tissue into the mass spectrometer provides very rich mass spectra with respect to the number of ions, so a high-resolution mass detector is needed for exact identification of the ions.
All experiments were performed in accordance with the guidelines of the Public Health Service Policy on Humane Care and Use of Laboratory Animals and the Ethical Committees of all institutions that have approved this research. Porcine eyes from 2 year old animals were provided by a local abattoir (LSO Foods Oy, Lahti, Finland) and transported to the laboratory within 6 h of sacrifice. The ocular lenses were immediately excised and stored in a physiological saline solution at 4°C for transportation to the MS laboratory. The tissues were frozen over liquid nitrogen and stored at −80°C.
For the MALDI analyses, the tissues were cut in a microcryotome (Leica CM 1950, Leica Biosystem, Germany) along the equatorial plane to generate 12 µm slices. The slices were then transferred and attached onto an ITO glass slide coated with a thin layer of ethanol (2 µL). The lens structure is extremely fragile when cut with a microcryotome into thin slices, so ethanol  or methanol ,  soft-landing procedures for the tissue on the MALDI surface have been used to fix the tissue structure for MALDI MSI analysis of proteins. Our previous work on sphingolipids has demonstrated that the use of ethanol does not affect the spatial distribution of lipids . After drying the samples for 10 min in a desiccator, the tissue was coated with α-cyano-4-hydroxycinnamic acid (CHCA) MALDI matrix using an ImagePrep (Bruker Daltonics, Germany) device. CHCA was prepared in 50/50% (v/v) acetonitrile/trifluoroacetic acid (0.2%) at a concentration of 7 mg/mL. A Nikon scanner (Coolscan VED, Nikon, Tokyo, Japan) was used for optical scanning of the tissues. The samples were analyzed immediately after MALDI matrix deposition.
For the UPLC-QTOFMS analyses, a standard mixture 1 (10 µl) containing PC(17∶0/0∶0), PC(17∶0/17∶0), PE(17∶0/17∶0) and Cer(d18∶1/17∶0), (Avanti Polar Lipids, Inc.) and TG(17∶0/17∶0/17∶0) (Larodan Fine Chemicals) was added to the lens samples before homogenization The samples were homogonised, with the HPLC-grade chloroform and methanol (3∶1; 3000 µL). The homogenate was mixed with 1.5 ml of 0.15 M NaCl (0.9%), vortexed for 1 min, and allowed to stand for 30 min. Subsequently, samples were centirfuged and the lower phase was collected and internal standard mixture 2 is added. The internal standard mixture 2 contained the labeled lipids PC (16∶1/0∶0-D3), PC(16∶1/16∶1-D6) and TG(16∶0/16∶0/16∶0-13C3).
MALDI-MS images were acquired by an APEX Ultra 9.4 T FT-ICR (dual ion source ESI/MALDI, Bruker Daltonics, Germany) mass spectrometer equipped with a Smart beam laser (200 Hz, spot diameter 50 µm). The entire area of the porcine lens was examined with the laser with a raster step size of 150 µm. The laser performed 600 shots per spot and single spectra were collected from one spot. The mass spectra were acquired in positive ion mode and the mass range was 200–1100 m/z. The mass resolution at 400 m/z was 66,000. The time fill for the ICR cell was 1400 µs. After analysis, the spectra were apodized using square sin apodization with one zero fill. Analysis of the entire tissue lasted about 8 h, and the resulting dataset was approximately 10 GB in size. The molecular images of the lipids were visualized using the FlexImaging software (version 2.1, Bruker Daltonics, Germany), and the intensity of the image was normalized to the total ion chromatogram. Identification of lipids was performed from the average spectra of the entire lens using Mass data analysis software . First, the spectra were internally calibrated against the five selected cluster ions of the CHCA MALDI matrix, and the mass peaks were deisotoped and then searched within an internal database adopted from the LIPID MAPS database . The tolerance for the search was 2 ppm, and protonated ions and sodium and potassium adducts were included. The local intensity of a lipid species was determined by a local Mean Gray Value at a grayscale molecular image in ImageJ image processing software (National Institutes of Health, USA, rsbweb.nih.gov/ij/) using the function Measure. The relative abundance of a lipid was calculated from the mass peak intensities of all identified lipids in the averaged mass spectra. In cases where a lipid was presented in multiple ion forms (e.g., as a protonated ion and/or sodium and potassium adducts), their intensities were summed. The lipid abundances were normalized to the most abundant peak in the mass spectra. Note that different lipid classes have different responses in MALDI, and it is unfortunately not feasible to quantify lipids directly from a tissue. Nevertheless, the measured intensities were in accordance with previously reported values , .
Lipid profiling by UPLC-QTOFMS
The lens lipid extracts were analyzed on a Waters Q-Tof Premier mass spectrometer combined with an Acquity Ultra Performance LC™ (UPLC). The column (at 50°C) was an Acquity UPLC™ BEH C18 2.1×100 mm with 1.7 µm particles. The solvent system included (A) ultrapure water (1% 1 M NH4Ac, 0.1% HCOOH) and (B) LC/MS grade acetonitrile/isopropanol (1∶1, 1% 1 M NH4Ac, 0.1% HCOOH). The gradient started from 65% A/35% B, reached 80% B in 2 min, 100% B in 7 min, and remained there for 7 min. The flow rate was 0.400 ml/min and the injected amount was 2.0 µl (Acquity Sample Organizer, at 10°C). Reserpine was used as the lock spray reference compound. The lipid profiling was carried out using ESI in positive mode and the data was collected at a mass range of m/z 300–1200 with scan duration of 0.2 sec.
The data processing using MZmine2 software included alignment of peaks, peak integration, normalization, and peak identification. Lipids were identified using an internal spectral library. The data was normalized using one or more internal standards representatives of each class of lipid present in the samples: the intensity of each identified lipid was normalized by dividing it with the intensity of its corresponding standard and multiplying it by the concentration of the standard. All monoacyl lipids except cholesterol esters, such as monoacylglycerols and monoacylglycerophospholipids, were normalized with PC(17∶0/0∶0), all diacyl lipids except ethanolamine phospholipids were normalized with PC(17∶0/17∶0), all ceramides with Cer(d18∶1/17∶0), all diacyl ethanolamine phospholipids with PE(17∶0/17∶0), and TG and cholesterol esters were normalized with TG(17∶0/17∶0/17∶0). Other (unidentified) molecular species were normalized with PC(17∶0/0∶0) for retention time <300 s, PC(17∶0/17∶0) for retention time between 300 s and 410 s, and TG(17∶0/17∶0/17∶0) for higher retention times. Finally, the lipids were further normalized by dividing the normalized lipid concentration with the protein content of the sample.
Conceived and designed the experiments: JP SKW JMH. Performed the experiments: JP VV TH JMH. Analyzed the data: JP VV TH MV PN MS JMH. Contributed reagents/materials/analysis tools: JP VV TH MV PN MS RK VH SKW JMH. Wrote the paper: JP VV TH MV PN MS RK VH SKW JMH.
- 1. Delaye M, Tardieu A (1983) Short-range order of crystallin proteins accounts for eye lens transparency. Nature 302: 415–417.M. DelayeA. Tardieu1983Short-range order of crystallin proteins accounts for eye lens transparency.Nature302415417
- 2. van Leyen K, Duvoisin RM, Engelhardt H, Wiedmann M (1998) A function for lipoxygenase in programmed organelle degradation. Nature 395: 392–395.K. van LeyenRM DuvoisinH. EngelhardtM. Wiedmann1998A function for lipoxygenase in programmed organelle degradation.Nature395392395
- 3. Sane P, Tuomisto F, Wiedmer SK, Nyman T, Vattulainen I, et al. (2010) Temperature-induced structural transition in-situ in porcine lens - Changes observed in void size distribution. Biochim Biophys Acta-Biomembranes 1798: 958–965.P. SaneF. TuomistoSK WiedmerT. NymanI. Vattulainen2010Temperature-induced structural transition in-situ in porcine lens - Changes observed in void size distribution.Biochim Biophys Acta-Biomembranes1798958965
- 4. Borchman D, Delamere NA, McCauley LA, Paterson CA (1989) Studies on the distribution of cholesterol, phospholipid, and protein in the human and bovine lens. Lens Eye Toxic Res 6: 703–724.D. BorchmanNA DelamereLA McCauleyCA Paterson1989Studies on the distribution of cholesterol, phospholipid, and protein in the human and bovine lens.Lens Eye Toxic Res6703724
- 5. Byrdwell WC, Borchman D, Porter RA, Taylor KG, Yappert MC (1994) Separation and characterization of the unknown phospholipid in human lens membranes. Invest Ophthalmol Vis Sci 35: 4333–4343.WC ByrdwellD. BorchmanRA PorterKG TaylorMC Yappert1994Separation and characterization of the unknown phospholipid in human lens membranes.Invest Ophthalmol Vis Sci3543334343
- 6. Mulders SM, Preston GM, Deen PM, Guggino WB, van Os CH, et al. (1995) Water channel properties of major intrinsic protein of lens. J Biol Chem 270: 9010–9016.SM MuldersGM PrestonPM DeenWB GugginoCH van Os1995Water channel properties of major intrinsic protein of lens.J Biol Chem27090109016
- 7. Rujoi M, Estrada R, Yappert MC (2004) In situ MALDI-TOF MS regional analysis of neutral phospholipids in lens tissue. Anal Chem 76: 1657–1663.M. RujoiR. EstradaMC Yappert2004In situ MALDI-TOF MS regional analysis of neutral phospholipids in lens tissue.Anal Chem7616571663
- 8. Li LK, So L, Spector A (1985) Membrane cholesterol and phospholipid in consecutive concentric sections of human lenses. J Lipid Res 26: 600–609.LK LiL. SoA. Spector1985Membrane cholesterol and phospholipid in consecutive concentric sections of human lenses.J Lipid Res26600609
- 9. Vidova V, Pol J, Volny M, Novak P, Havlicek V, et al. (2010) Visualizing spatial lipid distribution in porcine lens by MALDI imaging high-resolution mass spectrometry. J Lipid Res 51: 2298–2302.V. VidovaJ. PolM. VolnyP. NovakV. Havlicek2010Visualizing spatial lipid distribution in porcine lens by MALDI imaging high-resolution mass spectrometry.J Lipid Res5122982302
- 10. Heeren RM, Smith DF, Stauber J, Kukrer-Kaletas B, MacAleese L (2009) Imaging mass spectrometry: hype or hope? J Am Soc Mass Spectrom 20: 1006–1014.RM HeerenDF SmithJ. StauberB. Kukrer-KaletasL. MacAleese2009Imaging mass spectrometry: hype or hope?J Am Soc Mass Spectrom2010061014
- 11. Seeley EH, Caprioli RM (2008) Molecular imaging of proteins in tissues by mass spectrometry. Proc Natl Acad Sci U S A 105: 18126–18131.EH SeeleyRM Caprioli2008Molecular imaging of proteins in tissues by mass spectrometry.Proc Natl Acad Sci U S A1051812618131
- 12. Cornett DS, Reyzer ML, Chaurand P, Caprioli RM (2007) MALDI imaging mass spectrometry: molecular snapshots of biochemical systems. Nat Methods 4: 828–833.DS CornettML ReyzerP. ChaurandRM Caprioli2007MALDI imaging mass spectrometry: molecular snapshots of biochemical systems.Nat Methods4828833
- 13. Wiseman JM, Ifa DR, Song Q, Cooks RG (2006) Tissue imaging at atmospheric pressure using desorption electrospray ionization (DESI) mass spectrometry. Angew Chem Int Ed Engl 45: 7188–7192.JM WisemanDR IfaQ. SongRG Cooks2006Tissue imaging at atmospheric pressure using desorption electrospray ionization (DESI) mass spectrometry.Angew Chem Int Ed Engl4571887192
- 14. Fletcher JS (2009) Cellular imaging with secondary ion mass spectrometry. Analyst 134: 2204–2215.JS Fletcher2009Cellular imaging with secondary ion mass spectrometry.Analyst13422042215
- 15. Wiseman JM, Ifa DR, Zhu Y, Kissinger CB, Manicke NE, et al. (2008) Desorption electrospray ionization mass spectrometry: Imaging drugs and metabolites in tissues. Proc Natl Acad Sci U S A 105: 18120–18125.JM WisemanDR IfaY. ZhuCB KissingerNE Manicke2008Desorption electrospray ionization mass spectrometry: Imaging drugs and metabolites in tissues.Proc Natl Acad Sci U S A1051812018125
- 16. Ostrowski SG, Van Bell CT, Winograd N, Ewing AG (2004) Mass spectrometric imaging of highly curved membranes during Tetrahymena mating. Science 305: 71–73.SG OstrowskiCT Van BellN. WinogradAG Ewing2004Mass spectrometric imaging of highly curved membranes during Tetrahymena mating.Science3057173
- 17. Chughtai K, Heeren RM (2010) Mass spectrometric imaging for biomedical tissue analysis. Chem Rev 110: 3237–3277.K. ChughtaiRM Heeren2010Mass spectrometric imaging for biomedical tissue analysis.Chem Rev11032373277
- 18. McDonnell LA, Heeren RMA (2007) Imaging mass spectrometry. Mass Spectrometry Rev 26: 606–643.LA McDonnellRMA Heeren2007Imaging mass spectrometry.Mass Spectrometry Rev26606643
- 19. Altelaar AFM, Luxembourg SL, McDonnell LA, Piersma SR, Heeren RMA (2007) Imaging mass spectrometry at cellular length scales. Nature Protocols 2: 1185–1196.AFM AltelaarSL LuxembourgLA McDonnellSR PiersmaRMA Heeren2007Imaging mass spectrometry at cellular length scales.Nature Protocols211851196
- 20. Deeley JM, Mitchell TW, Wei XJ, Korth J, Nealon JR, et al. (2008) Human lens lipids differ markedly from those of commonly used experimental animals. Biochim Biophys Acta Mol Cell Biol Lipids 1781: 288–298.JM DeeleyTW MitchellXJ WeiJ. KorthJR Nealon2008Human lens lipids differ markedly from those of commonly used experimental animals.Biochim Biophys Acta Mol Cell Biol Lipids1781288298
- 21. Borchman D, Yappert MC (2010) Lipids and the ocular lens. J Lipid Res 51: 2473–2488.D. BorchmanMC Yappert2010Lipids and the ocular lens.J Lipid Res5124732488
- 22. Estrada R, Yappert MC (2004) Regional phospholipid analysis of porcine lens membranes by matrix-assisted laser desorption/ionization time-of-flight mass spectrometry. Journal of Mass Spectrometry 39: 1531–1540.R. EstradaMC Yappert2004Regional phospholipid analysis of porcine lens membranes by matrix-assisted laser desorption/ionization time-of-flight mass spectrometry.Journal of Mass Spectrometry3915311540
- 23. Yappert MC, Rujoi M, Borchman D, Vorobyov I, Estrada R (2003) Glycero-versus sphingo-phospholipids: correlations with human and non-human mammalian lens growth. Exp Eye Res 76: 725–734.MC YappertM. RujoiD. BorchmanI. VorobyovR. Estrada2003Glycero-versus sphingo-phospholipids: correlations with human and non-human mammalian lens growth.Exp Eye Res76725734
- 24. Deeley JM, Hankin JA, Friedrich MG, Murphy RC, Truscott RJ, et al. (2010) Sphingolipid distribution changes with age in the human lens. J Lipid Res 51: 2753–2760.JM DeeleyJA HankinMG FriedrichRC MurphyRJ Truscott2010Sphingolipid distribution changes with age in the human lens.J Lipid Res5127532760
- 25. Ellis SR, Wu C, Deeley JM, Zhu X, Truscott RJ, et al. (2010) Imaging of Human Lens Lipids by Desorption Electrospray Ionization Mass Spectrometry. J Am Soc Mass Spectrom 21: 2095–2104.SR EllisC. WuJM DeeleyX. ZhuRJ Truscott2010Imaging of Human Lens Lipids by Desorption Electrospray Ionization Mass Spectrometry.J Am Soc Mass Spectrom2120952104
- 26. Cantor RS (1999) Solute modulation of conformational equilibria in intrinsic membrane proteins: apparent “Cooperativity” without binding. Biophys J 77: 2643–2647.RS Cantor1999Solute modulation of conformational equilibria in intrinsic membrane proteins: apparent “Cooperativity” without binding.Biophys J7726432647
- 27. Han J, Schey KL (2006) MALDI tissue Imaging of ocular lens alpha-crystallin. Invest Ophthalmol Vis Sci 47: 2990–2996.J. HanKL Schey2006MALDI tissue Imaging of ocular lens alpha-crystallin.Invest Ophthalmol Vis Sci4729902996
- 28. Grey AC, Chaurand P, Caprioli RM, Schey KL (2009) MALDI Imaging Mass Spectrometry of Integral Membrane Proteins from Ocular Lens and Retinal Tissue. J Proteome Res 8: 3278–3283.AC GreyP. ChaurandRM CaprioliKL Schey2009MALDI Imaging Mass Spectrometry of Integral Membrane Proteins from Ocular Lens and Retinal Tissue.J Proteome Res832783283
- 29. Grey AC, Schey KL (2009) Age-Related Changes in the Spatial Distribution of Human Lens alpha-Crystallin Products by MALDI Imaging Mass Spectrometry. Invest Ophthalmol Vis Sci 50: 4319–4329.AC GreyKL Schey2009Age-Related Changes in the Spatial Distribution of Human Lens alpha-Crystallin Products by MALDI Imaging Mass Spectrometry.Invest Ophthalmol Vis Sci5043194329
- 30. Strohalm M, Kavan D, Novak P, Volny M, Havlicek V (2010) mMass 3: A Cross-Platform Software Environment for Precise Analysis of Mass Spectrometric Data. Anal Chem 82: 4648–4651.M. StrohalmD. KavanP. NovakM. VolnyV. Havlicek2010mMass 3: A Cross-Platform Software Environment for Precise Analysis of Mass Spectrometric Data.Anal Chem8246484651
- 31. Lipid Maps consortium website. Lipid Maps consortium website.Available: www.lipidmaps.org. Accessed 2011 Mar 6. Available: www.lipidmaps.org. Accessed 2011 Mar 6.
- 32. Huang L, Grami V, Marrero Y, Tang DX, Yappert MC, et al. (2005) Human lens phospholipid changes with age and cataract. Invest Ophthalmol Vis Sci 46: 1682–1689.L. HuangV. GramiY. MarreroDX TangMC Yappert2005Human lens phospholipid changes with age and cataract.Invest Ophthalmol Vis Sci4616821689