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### Summary

Non-stirred precipitation polymerization provides a rapid, reproducible prototyping approach to the synthesis of stimuli-sensitive poly(*N*-isopropylacrylamide) microgels of narrow size distribution. In this protocol synthesis, light scattering characterization and single particle fluorescence tracking of these microgels in a wide-field microscopy setup are demonstrated.

### Cite this Article

Copy Citation | Download CitationsVirtanen, O. L., Purohit, A., Brugnoni, M., Wöll, D., Richtering, W. Controlled Synthesis and Fluorescence Tracking of Highly Uniform Poly(*N*-isopropylacrylamide) Microgels. *J. Vis. Exp.* (115), e54419, doi:10.3791/54419 (2016).

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### Abstract

Stimuli-sensitive poly(*N*-isopropylacrylamide) (PNIPAM) microgels have various prospective practical applications and uses in fundamental research. In this work, we use single particle tracking of fluorescently labeled PNIPAM microgels as a showcase for tuning microgel size by a rapid non-stirred precipitation polymerization procedure. This approach is well suited for prototyping new reaction compositions and conditions or for applications that do not require large amounts of product. Microgel synthesis, particle size and structure determination by dynamic and static light scattering are detailed in the protocol. It is shown that the addition of functional comonomers can have a large influence on the particle nucleation and structure. Single particle tracking by wide-field fluorescence microscopy allows for an investigation of the diffusion of labeled tracer microgels in a concentrated matrix of non-labeled microgels, a system not easily investigated by other methods such as dynamic light scattering.

### Introduction

Stimuli-sensitive poly(*N*-isopropylacrylamide) (PNIPAM) microgels ^{1,2} have attracted continuous interest over the past two decades due to their potential in various smart applications. Demonstrated use cases include switchable emulsion stabilizers ^{3-8}, microlenses^{ 9}, cell culture substrates for easy cell harvesting ^{10,11}, and smart carriers for low molecular weight compounds and other biomedical uses ^{12}. From a fundamental research point of view these particles have been proven to be useful for investigating subjects such as colloidal interactions ^{13-15} and polymer-solvent interactions ^{16-18}.

Successful use of PNIPAM microgels and their derivatives in any given application typically requires knowledge on the mean particle size and width of the particle size distribution. For the correct interpretation of the experimental results involving PNIPAM microgels, the particle structure, which can be affected by functional comonomers, has to be known. Dynamic and static light scattering (DLS and SLS, respectively) are uniquely suited for acquiring this information because these methods are fast and relatively easy to use; and they probe the particle properties non-invasively in their native environment (dispersion). DLS and SLS also collect data from vast number of particles avoiding the bias arising from small sample sizes, typical for microscopy methods. Therefore, the first aim of this work is to introduce good practice regarding light scattering for practitioners new to colloidal characterization.

Typically, precipitation polymerization is carried out in laboratory scale and finding the right reaction conditions for specific particle properties can be laborious and require many repetitions of the synthesis. In contrast to large batch synthesis, non-stirred precipitation polymerization ^{19,20} is a rapid procedure in which batches of different reactant composition can be polymerized simultaneously yielding particles of narrow size distribution. Simultaneous polymerization minimizes experimental variation and large output means that right reaction conditions can be found fast for upscaling the reaction. Hence, our second aim is to demonstrate the usefulness of non-stirred precipitation polymerization in prototyping and in applications that do not require a large amount of product.

Different aspects of synthesis and characterization come together in the example of application of fluorescent labeled PNIPAM microgels in colloidal interaction research. Here we use highly accurate single particle tracking to investigate the diffusion of labeled tracer microgels in dispersion of unlabeled matrix microgels over a wide matrix concentration range and resolve the cage effect in concentrated colloidal dispersion. Wide-field fluorescence microscopy is well suited for this purpose as it can characterize the specific behavior of a few tracer molecules among a large number of potentially different matrix species. This is in contrast to techniques such as DLS, SLS and rheology, which measure the ensemble average properties of systems and therefore cannot resolve behavior of small number of probe particles in a large system. Furthermore, in this specific example conventional light scattering methods cannot be utilized also due to high particle concentration, which leads to strong multiple scattering invalidating any standard analysis. Use of automated data processing and statistical methods enable analysis of overall system behavior also for single particle tracking, when averaged over large sample sizes.

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### Protocol

1. Microgel Synthesis

NOTE: *N*-isopropylacrylamide (NIPAM) was recrystallized from n-hexane. Other reagents were used as received.

- Conventional Batch Synthesis of Poly(NIPAM) Matrix Microgels
- Dissolve 1.8 g NIPAM and 24 mg
*N,N'*-bisacrylamide (BIS) in 245 ml filtered (0.2 µm regenerated cellulose (RC) membrane filter) double distilled water in a 500 ml three-neck round bottom flask equipped with a reflux condenser, a stirrer and a rubber septum. - Insert a thermometer and a 120 mm needle for the nitrogen input through the septum.
- Heat the solution to 60 °C, while stirring. Deoxygenate the solution by purging with nitrogen for 40 min.
- Simultaneously prepare an initiator solution of 155 mg potassium persulfate (KPS) in 5 ml filtered double-distilled water and bubble the solution with nitrogen to remove oxygen.
- Transfer the complete 5 ml KPS solution in a nitrogen-washed syringe equipped with a 120 mm needle.
- Lift the nitrogen needle above the solution level in the three-neck flask and add the KPS solution rapidly through the rubber septum into the reactor.
- Let the polymerization proceed for 1 hr under nitrogen flow and slow stirring at 60 °C.
- Use a Buchner funnel and filter paper to filter the hot reaction solution in order to discard big aggregates. Let the dispersion to cool down.
- Centrifuge and redisperse the dispersion three times for 40 min at 257,000 x g and finally redisperse the sediment in a minimum viable amount of double distilled water. Typically this is 2-4 ml.
- Lyophilize the dispersion for storing.

- Dissolve 1.8 g NIPAM and 24 mg
- Non-stirred Synthesis of Fluorescently Labeled Poly(NIPAM) Microgels
- Weigh 257.7 mg NIPAM, 3.5 mg BIS, and 1.5 mg methacryloxyethyl thiocarbamoyl rhodamine B (dye) in glass vessel and add 10 ml of filtered double distilled water.
- Ultrasonicate the dye–monomer solution for 15 min to dissolve the dye in water.
- Prepare the same solution without the dye into a separate glass vessel.
- Prepare various dilutions of the monomer solution with the dye using the monomer solution without the dye to obtain a concentration series with various dye concentrations. In this work, use dye in the concentration range of 0.02-0.1 mmol/L.
- Dissolve 8.4 mg KPS in 10 ml filtered double distilled water in order to get the initiator solution.
- Transfer 0.5 ml of the concentration series and 0.5 ml of the KPS solution to test tubes with 10 mm diameter to obtain the final reaction solutions and seal them with rubber septa.
- Preheat an oil bath in a double-walled glass vessel connected to a heating circulator to 63 °C.
- Deoxygenize the reaction solutions by purging with nitrogen through 120 mm needles for 20 min.
- Insert the tubes into a floating platform and immerse the platform into the preheated oil bath. Set the temperature to 60 °C. Initially higher temperature in the bath is necessary as the room temperature solutions cool down the bath. For high precision particle size tuning the temperature control during the initial reaction has to be rigorous, typically ±0.1 °C.
- Let the reaction proceed for an appropriate time. Typically 1 hr is enough.
- Transfer the reaction tubes rapidly to an oven at 60 °C and put one drop of the hot dispersion to 10 ml filtered double distilled water preheated over PNIPAM volume phase transition temperature (VPTT, 32 -34 °C)
^{1}, for DLS characterization in the collapsed state. - Let the rest of the dispersions cool down to room temperature and transfer them into centrifuge tubes.
- Centrifuge the solution three times for 40 min at 257,000 x g and dilute the microgels finally in 2 ml filtered double distilled water for use as tracer particles.

2. Light Scattering Characterization

- Hydrodynamic Radius Determination in Collapsed State by Dynamic Light Scattering
- Wash cuvettes and glassware with acetone vapor.
- Heat 10 ml of filtered (
*e.g.,*200 nm or smaller RC filter) double distilled water over PNIPAM VPTT. - Transfer a drop of hot dispersion to the filtered water using a pre-heated needle (0.9 x 40 mm) and syringe (1 ml).
- Temper the DLS goniometer index match bath to 50 °C and transfer the sample to the instrument without letting it cool down.
- Find the largest scattering angle where the scattered intensity is sufficient to acquire a correlogram by performing test measurements.
- Insert sample cuvette (10 mm diameter glass tube with 1 ml of particle dispersion). Move the detector arm to small scattering angle (here 30°).
- Check the beam profile for multiple scattering: no glow around the primary beam, no multiple scattering,
*etc.*Check that the count range is suitable for measurement at the lowest scattering angle (approx. between 30 and 600 kHz; top right corner of the software window.) - Move the goniometer arm to highest scattering angle (choose 120° here). Check that the count rate is still high enough for the measurement (between 30 and 600 kHz). If the intensity is too low, move the arm to lower scattering angle.

- Check the beam visually through the toluene bath glass at the lowest scattering angle, if glow around the incident beam is observed multiple scattering takes place. In this case, reduce the laser intensity or use a higher dilution.
- Acquire 20 correlograms between the minimum and maximum scattering angle (
*e.g.*, 30° - 140°) with minimum acquisition time of 60 sec. Increase the acquisition time for weak intensity large scattering angles if necessary.

- Data Analysis
^{37}- Calculate scattering vector magnitudes for the scattering angle according to , where
*n*is the refractive index of the dispersion, the wavelength of the laser in vacuum and the scattering angle. - In the case the measurement software provides the intensity correlation function , transform it to electric field correlation function according to . Parameter is an uninteresting instrumental parameter related to the degree of spatial coherence of the scattered light over the detector area.
- Perform cumulant analysis on correlograms,
*i.e.*, fit second order polynomial to the logarithm of each electric field correlation function by linear least squares. appears as the intercept of the fit and its exact value is unimportant in respect to the data analysis. Restrict the fit to a meaningful lag time*τ*value,*e.g.*, so that the correlation amplitude is 10 - 20 % of the maximum amplitude. The coefficient of the first order term is the mean decay rate of the correlation function, . - Find the most likely value for the mean diffusion coefficient of the particles by linear least squares fit on . If against does not appear linear and go through the origin within the error, the particle size distribution is broad and hydrodynamic radius will be poorly defined.
- Calculate the mean hydrodynamic radius from the Stokes-Einstein relation
*,*where is the Boltzmann coefficient, the absolute temperature and the viscosity of the dispersion at . Propagate the standard deviation of to .

- Calculate scattering vector magnitudes for the scattering angle according to , where
- Particle Structure Determination by Static Light Scattering
- Wash cuvettes and glassware with acetone vapor. Use 20 mm diameter or larger cuvettes to minimize the cylindrical lens effect.
- Filter (200 nm RC filter or smaller) approximately 20 ml of double distilled water to a glass vial and transfer a drop of purified dispersion to the vial. Wash the filter with 10 ml water before using it for sample preparation to remove impurities remaining from the manufacturing process.
- Check sample against any ambient light source. If blue hue is observed, the sample is likely to be too concentrated. Dilute accordingly.
- Prepare background water sample by flushing the cuvette multiple times with filtered water and then fill up to appropriate sample volume, depending on the cuvette and the laser position in the instrument. The laser must pass through the sample without being refracted from the meniscus.
- Calibrate the instrument using a toluene sample.
- Measure water scattering (background) throughout the available angular range.
- Measure the scattering intensity from the sample throughout the available angular range preferably at several wavelengths. The scattering pattern normalized to the forward scattering intensity is known as the form factor.
- If particle structure is known, use the appropriate model expression to calculate global fit on the datasets measured at different wavelengths.
- For unknown particle structure use regularized direct (such as FitIt!
^{33}) or a more general indirect inverse Fourier transform^{21,22}routine in conjunction with deconvolution of the pair distance distribution function (only for spherical particles)^{23,24}for approximate classification of particle type. - In case the fitting or inversion routine provides an estimate of the particle radius distribution function, calculate the polydispersity index (standard deviation of the distribution divided by its mean).

3. Particle Tracking by Wide-field Fluorescence Microscopy

NOTE: Tracer and matrix particles of 465 ± 7 nm and 405 ± 7 nm hydrodynamic radii at 20 °C, respectively, were used for particle tracking.

- Sample Preparation
- Prepare concentrated matrix microgel dispersion by redispersing known amount of lyophilized unlabeled microgel to known amount of double distilled water. Add a small volume of labeled tracer particles.
- Confirm the appropriate tracer microgel concentration in the microscope. The optimal concentration is a compromise between simultaneous acquisitions of maximum number of tracks, while having the tracer concentration low enough so that the probability that the tracer particle tracks cross during the acquisition is negligible.
- Prepare concentrated dispersions by evaporating water in an oven. Determine weight concentration by comparing the weight of the dispersion to the original weight of the sample before evaporation.

- Data Acquisition and Analysis
- Use an appropriate objective lens of the desired magnification and aperture for excitation of the tracers and simultaneous fluorescence collection from the sample. In this work, use a 100X/1.3 NA oil immersion objective lens.
- Place the moisture chamber onto a xyz-piezo table, which fits into a commercial microscope.
- To prevent the sample from drying, place a plasma cleaned cover slip into the moisture chamber and pipette 10 µl of poly(NIPAM) dispersion of the desired concentration onto the slip.
- Depending on the excitation and emission spectra of the fluorescent dye, use a suitable laser for excitation and adjust the laser power appropriately. The intensity should be sufficiently low to avoid fast photobleaching of the dyes, but at the same time strong enough for accurate single particle positioning (see below). In this work, use a 561 nm diode-pumped solid-state laser and keep the laser power constant at 16 mW (
*ca.*0.5 kW cm^{-2}at the sample) for all the measurements. - To obtain homogeneous sample illumination, use the critical illumination setup described here. For this, couple the laser into a multimode fiber (NA 0.22 ± 0.02, 0.6 mm core diameter), shake the fiber using a vortexer in order to temporally average out laser speckles, and project the fiber end into the sample plane.
- Calibrate the z distance from the back reflection of the cover slip and focus several micrometers into the sample by moving the objective slightly up and fix the z-position using a z-compensator. This avoids any interface effects with the coverslip.
- Adjust the detector parameters, such as exposure time, to the strength of the fluorescence signal. In this case, use an EMCCD camera with exposure time of 0.1 sec, electron multiplying mode and gain of 50.
- Acquire several movies with the appropriate number of frames to obtain adequate lag time to calculate the mean square displacement of the microgels in different regions of the sample. In this work, use acquisition frame numbers of 500 or 1,000 frames.
- Analyze the data by positioning the particles in each frame using Gaussian fitting
^{25}and use an appropriate particle tracking algorithm^{26}to obtain the mean square displacement.^{27}Calculate mean values and standard deviation by averaging over all the tracks in all the movies. Calculate the long lag time diffusion coefficients by linear regression from , where is the mean square displacement,*D*the mean diffusion coefficient and*τ*the lag time. - Estimate the anomaly parameter
*γ*from the anomalous diffusion equation by transforming the data to logarithmic scale, yielding . The anomaly parameter is given by the derivative of the plot. The derivative can be estimated by the finite differences of the data points, or fitting the data points by polynomial functions and differentiating analytically. Determine the sufficient degree of the polynomial fit functions by plotting the fit residuals and residual norm for increasing polynomial order. - Repeat the same procedure for different concentrations of the microgel matrices.

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### Representative Results

The number of PNIPAM microgel particles in the batch, and thus the final particle volume, is determined early in the reaction during the nucleation phase ^{20} Hydrophobic co-monomer dye methacryloxyethyl thiocarbamoyl rhodamine B influences the nucleation by reducing the particle number density in the batch. The decrease in particle concentration for two different initial NIPAM concentrations can be seen as increase in the mean final particle volume in the collapsed state with increasing dye concentration, shown in **Figure 1**. The increase in volume can be attributed to the hydrophobic comonomer dye, which promotes microgel nuclei aggregation at early reaction times, decreasing the particle concentration and increasing the final particle volume.

Results from a successful DLS measurements are shown in **Figure 2**. For the six smallest final particle volume batches linear dependence of the mean decay rate Γ_{2} on *q*^{2} and zero y-intercept within the error indicate that the particle size distributions for these batches are relatively narrow and a well-defined estimate for the mean diffusion coefficient can be obtained from the slope of the linear fit. **Figure 3** shows a more complicated result from the two largest volume batches, where Γ_{2} deviates from the linear behavior in the intermediate* q* range. The non-linearity originates from the form factor (angular scattering pattern) minimum which coincides with these *q *values. ^{28} The phenomenon in question can be observed for particles with dimensions comparable to the wavelength of the incident laser radiation and even a moderate particle size distribution width. Determination of diffusion coefficient in this *q* range results in strongly biased results and therefore poses a notable risk of mischaracterization. In the specific case of **Figure 3**, Γ_{2 }reflects the mean behavior again at high *q*, where all particle size fractions contribute more evenly to the total scattered intensity. A straightforward way to obtain a reasonable estimate for the mean diffusion coefficient is to exclude the intermediate Γ_{2 }values from the linear fit. If the form factor of the particles are known, a more elaborate fitting method can be used ^{28}.

Determining the hydrodynamic volume in the collapsed state without letting the samples cool down below the PNIPAM VPTT ensures that the non-gelled sol fraction has not detached from the particles. Therefore the volume in the collapsed state reflects the mass and the number of the particles during the polymerization, which is important if the fundamental properties of the precipitation polymerization are being investigated ^{20}. Volume in the collapsed state also provides a good quantity for comparing different reaction parameters, because it is independent of the swelling properties and the fraction of non-gelled polymer in the particles regulated by the amount of cross-linker in the monomer mixture. Smaller size and higher scattering contrast in the collapsed state also facilitate the DLS characterization.

Static light scattering data measured at two wavelengths of 642 nm and 404 nm for the matrix and tracer particles are shown in **Figure 4**. Visual inspection of the angular scattering patterns reveals that the particles are well-defined: Multiple distinguished oscillations typical for spherical particles throughout the *q* indicates narrow polydispersity, in this case 7% and 6% for the tracer and matrix microgels, respectively. Smooth behavior at low *q* indicates that the samples are sufficiently diluted and no significant particle aggregation is present. The increase in scattered intensity at extreme *q* can be attributed to the scattering due to the back reflected beam from the inner cuvette wall. Inversion of the form factors of the matrix particles confirm typical microgel structure ^{29} with dense core and radially decaying density profile resulting from cross-linker copolymerization kinetics ^{30} (see inset). The dashed line shows the form factor of the reference hard sphere with the same mean radius of gyration as the matrix particles. The experimental form factor decays faster with *q* than the hard sphere form factor, which is typical for particles with fuzzy surface. In contrast, tracer particles exhibit unconventional microgel structure. This can be also seen from the reference hard sphere form factor, which shows that the experimental form factor initially does not decay faster than the reference. This result shows that the incorporating dye molecules to microgels can affect their structure, which must be accounted for in interpretation of the results.

The high uniformity of the synthesized particles is of high interest for studies of their diffusion at volume fractions around the glass transition temperature in order to accurately determine the evolution behavior in this regime ^{13}, and compare it to hard particles ^{31}. Therefore, a low fraction of labeled microgels were mixed with non-labeled microgel of comparable size. Excitation and emission spectra of microgel-incorporated dye molecules along with the excitation wavelength and filter configuration used in the emission path are presented in **Figure 5**. Absorbance and emission maxima of methacryloxyethyl thiocarbamoyl rhodamine B are close to excitation wavelength and fluorescence collection range, respectively, enabling high collection efficiency in the particle tracking setup. The time evolution of mean square displacement for tracer microgels in various non-labeled microgel matrix concentrations are shown in **Figure 6** and **Figure 7** in linear and logarithmic scale, respectively. At low microgel matrix concentrations the tracer particles diffuse rapidly. Even though they are only visible for a limited number of frames before moving out of the focus plane, a reasonably good estimation of their mean square displacements is possible. The linear increase of the mean square displacement with time indicates normal diffusion behavior for all lag times measured. However, for microgel concentrations close to the colloidal glass transition, *i.e.,* 29-36 mg/ml, the temporal evolution of the mean square displacements becomes non-linear (see **Figure 7**). The behavior resembles the one of colloidal micrometer-sized PMMA particles as described by Weeks and Weitz ^{31} and can be related to the cage effect. As shown schematically in **Figure 10**, a labeled microgel in a dense matrix can diffuse rather freely within the cage. For that reason, the mean square displacement increases linearly in the first few milliseconds. However, since particles are trapped in transient cages formed by their neighbors, a collective rearrangement of the surrounding microgels is necessary for microgels to move further. This cage effect expresses itself in a rather shallow slope in the second range of **Figure 7**, and can be also confirmed by inspecting the particle tracks in **Figure 9**. At short lag times the particles jiggle in their cages, from which they escape just to get trapped again. At long lag times, the linear diffusion behavior is recovered. Cage effects can be analyzed using anomalous diffusion models where the temporal evolution of the (two-dimensionally detected) mean square displacement is expressed by a power law in time: or in its logarithmic form with the anomaly parameter * *^{32}. For normal diffusion, the anomaly parameter equals 1, subdiffusion is represented by values below 1. **Figure 8** presents the temporal evolution of the anomaly parameter directly determined from the slope in the log-log-plot **Figure 7**. For the lower concentrations of microgels in our study, the anomaly parameter basically equals to 1. For lag times in the range of several seconds, the factor deviates from 1 towards lower values. This behavior is an artifact due to fact that the axial (z-)observation range in wide-field microscopy is limited to only a few micrometers. The narrow z-range biases the analysis for fast diffusion at long time intervals for rapidly diffusing tracers at low matrix concentrations. When increasing the microgel concentration, we find that the minimum of the anomaly parameter becomes much more pronounced and the transition to normal diffusion () appears later. This is a clear indication of the cage effect appearing for dense microgels systems when approaching their glass transition regime.

**Figure 1:** **Single particle volume in collapsed state with initial dye concentration in the batch. **Two different initial NIPAM concentrations were used, 57.5 mmol dm^{-3} (black circles) and 28.8 mmol dm^{-3} (grey rectangles). 1 mol-% of cross-linker was used. Initial KPS concentration was the same in all the batches at 1.56 mmol dm^{-3}. Error bars denote the standard deviation. Please click here to view a larger version of this figure.

**Figure 2:** **Decay rate with the square of the scattering vector magnitude for the four smallest volume microgel batches.** Linear dependence of on *q*^{2 }and zero intercept indicate narrow particle size distribution and indicates that well-defined estimate of the mean diffusion coefficient can be calculated from the slope of the linear fit. NIPAM concentrations were 57.5 mmol dm^{-3} (red squares and orange inverted triangles) and 28.8 mmol dm^{-3} (rest of the symbols). Dye concentrations were 0.044 mmol dm^{-3} (red squares), 0.022 mmol dm^{-3} (orange inverted triangles), 0.088 mmol dm^{-3} (green triangles), 0.066 mmol dm^{-3} (cyan rhombuses), 0.044 mmol dm^{-3} (dark blue triangles), and 0.022 mmol dm^{-3} (pink circles). Please click here to view a larger version of this figure.

**Figure 3:** **Decay rate with the square of the scattering vector magnitude for the two largest volume batches. **Non-linear behavior of Γ_{2} with *q*^{2} in the central *q* range is caused by the changes in the intensity weighting of signal by different size fractions in the vicinity of the form factor minimum. NIPAM concentration in the both batches were 57.5 mmol dm^{-3}, the dye concentrations were 0.088 mmol dm^{-3 }(black circles) and 0.066 mmol dm^{-3} (red triangles). Faded symbols were excluded from the linear fit. Please click here to view a larger version of this figure.

**Figure 4:** **Form factors of the labeled tracer and unlabeled matrix particles.** For both particles the form factor was measured at two wavelengths, 642 nm (light blue and red data points) and 404 nm (green and dark blue data points). Solid lines are global fits to the 642 nm and 404 nm datasets. Dashed lines show form factors of hard sphere reference particles with the same radii of gyration as matrix and tracer particles (orange and green dashed lines, respectively.) Insets show normalized particle density profiles from the core to the surface calculated, *e.g.*, FitIt! Please click here to view a larger version of this figure.

**Figure 5:** **Excitation and emission spectra of fluorescence labeled microgel particles.** Blue line denotes the excitation and red line emission spectrum. Solid vertical line is the excitation wavelength. Shaded area denotes fluorescence collection wavelength range. Please click here to view a larger version of this figure.

**Figure 6:** **Mean square displacement with lag time for the tracer particles.** Unlabeled matrix microgel concentrations were 15.56 mg/ml (left), 22.05 mg/ml, 28.28 mg/ml, 28.67 mg/ml, 30.32 mg/ml, 31.13 mg/ml and 35.35 mg/ml. Points and error bars denote experimental values and standard deviation, respectively. Solid lines are linear fits to the data points. Inset shows a wide-field fluorescence micrograph of tracer microgels at 35.35 mg/ml matrix concentration. Please click here to view a larger version of this figure.

**Figure 7:** **Mean square displacement with lag time for the tracer particles in logarithmic scale. **Unlabeled matrix microgel concentrations were 15.56 mg/ml (left), 22.05 mg/ml, 28.28 mg/ml, 28.67 mg/ml, 30.32 mg/ml, 31.13 mg/ml and 35.35 mg/ml. Points and error bars denote experimental values and standard deviation, respectively. Solid lines are polynomial fits to the data points. Please click here to view a larger version of this figure.

**Figure 8:** **Anomaly parameters with lag time for tracer particles.** Unlabeled matrix microgel concentrations were 15.56 mg/ml (left), 22.05 mg/ml, 28.28 mg/ml, 28.67 mg/ml, 30.32 mg/ml, 31.13 mg/ml and 35.35 mg/ml. Points represent derivatives estimated by finite differences and solid lines analytically calculated derivatives from the polynomial fits in Figure 7. Please click here to view a larger version of this figure.

**Figure 9: Particle tracks for 12 tracer microgels in dispersion with 35.35 mg/ml matrix concentration.** Clustering of tracks to distinctive blobs results from the tracer's particles being trapped in transient cages formed by their unlabeled neighbors. Please click here to view a larger version of this figure.

**Figure 10:** **Schematic illustration of tracer microgel diffusion in concentrated unlabeled matrix microgel dispersion.** Red trajectory denotes rapid diffusion of the tracers within the transient cages (blue dashed line) formed by the neighboring particles. Blue trajectory denotes long lag time diffusion enabled by the collective rearrangement of the transient cages. Please click here to view a larger version of this figure.

**Figure 11:** **Long lag time diffusion coefficients with unlabeled matrix microgel concentration.** At low matrix concentration the diffusion of the tracer microgels is not affected by the matrix particles. With increasing matrix microgel concentration the long time diffusion slows down orders of magnitude because diffusion requires collective rearrangement of the transient cages, where the tracers are trapped. Please click here to view a larger version of this figure.

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### Discussion

Addition of small amounts of functional comonomer can have a significant effect on the particle size and structure of the PNIPAM derived microgels. Simultaneous small-scale test tube polymerization is a good method to account for such changes, and helps to rapidly find the right reactant compositions for target particle size for upscaling the reaction as needed. The mass of the particles is approximately exponentially dependent on the polymerization temperature when thermally decomposing initiator, such as KPS, is used^{ 20}, and therefore one needs to establish stable and accurate temperature control inside the reactor for good reproducibility. Final particle volumes from conventional batch reaction and non-stirred reaction are typically in good agreement if one minimizes batch synthesis related perturbations, such as too violent stirring of the reaction mixture to even out temperature gradients in the large reactor, or using excessive amount of initiator solution so that the reaction temperature changes during the initiation period.

Dynamic light scattering is a well-established and fast method to determine diffusion behavior of large number of particles *in situ*. It is however essential to acquire data at multiple scattering angles. DLS measurements at one arbitrary angle, coinciding with a form factor minimum or in the case of broad size distribution, will lead to an apparent diffusion coefficient significantly differing from the mean diffusion coefficient of the sample. Such cases can be recognized from non-linear behavior in Γ_{2} vs. *q*^{2} plot. For resolving broad or multimodal particle size distributions, one can attempt to use an inverse Laplace transformation algorithm such as CONTIN^{34}. DLS is however not ideally suited for this purpose due to ill-conditioned nature of the inversion problem.

For both dynamic and static light scattering the samples have to be sufficiently diluted to avoid multiple scattering, which invalidates the routine data analysis. For form factor determination by SLS also the refractive index difference of the particles and solvent has to be low in order to avoid Mie scattering, which prevents straightforward form factor analysis. This condition is fulfilled when , where is the mean particle radius and the difference between refractive indices of solvent and particles. For microgels extensively swollen with solvent this criterion is fulfilled, but in general the particles have to be contrast matched with sufficiently high refractive index solvent. Mie scattering can be recognized from the smearing of the form factor minima, an effect, which diminishes when the refractive index difference decreases.

Light scattering methods provide ensemble averaged information, whereas wide-field particle tracking can be used to investigate the diffusion behavior of single particles in real space. In contrast to particle tracking based on light scattering, the high sensitivity of fluorescence allows for tracking of small particles and, in the extreme case, even single molecules. Additionally, the ratio of labeled and non-labeled particles can be adapted to measure accurately also in highly concentrated solutions. Particle tracking therefore provides a model free way to determine the diffusion coefficient and diffusion mode of colloids *in situ* even allowing for a comparison between the behaviors of single particles. Localization accuracy of single tracers is typically better than the diffraction limit but depends on the signal-to-noise-ratio of the fluorescence signal of single particles on the wide-field setup. Thus, labeling with dyes that exhibit a high quantum yield, good photostability and an absorption maximum close to the excitation wavelength is a prerequisite for good results. Tracer concentration has to be kept low in order to minimize crossing of the trajectories of different particles disturbing the tracking algorithm. For concentrated dispersions, the density of fluorescent tracers can be adjusted by mixing labeled and non-labeled particles. Recent work on point spread function engineering enables 3D particle tracking ^{35,36}, which can be used to investigate anisotropic diffusion in different directions of space.

In summary, accurate DLS characterization and small-scale test tube polymerization provide robust framework for high precision tuning of microgel final particle volume. Light scattering and fluorescence particle tracking techniques provide complementary information on the ensemble and single particle diffusion behavior over wide dispersion concentration range. The combination of the synthesis of well-defined soft particles with the possibility to track them in solutions of different concentration will be of significant importance for the investigation of the dynamics of soft particle systems and a comparison with well-studied hard colloid systems.

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### Disclosures

The authors have nothing to disclose.

### Acknowledgments

The Deutsche Forschungsgemeinschaft (DFG) is acknowledged for financial support within the Sonderforschungsbereich SFB 985 "Functional Microgels and Microgel Systems".

### Materials

Name |
Company |
Catalog Number |
Comments |

Acetone | VWR Chemicals | KRAF13455 | |

Bisacrylamid | AppliChem | A3636 | |

n-Hexane | Merck | 104374 | |

N-Isopropylacrylamide |
Fisher Scientific | AC412785000 | recrystallized from n-hexane |

Methacryloxyethyl thiocarbamoyl rhodamine B | Polysciences | 23591 | |

Potassium peroxodisulfate | Merck | 105091 | |

Silicone oil 47 V 350 | VWR Chemicals | 83851 | |

Toluene | Sigma Aldrich | 244511 | |

F12 Refrigerated/heating circulator | Julabo | 9116612 | |

Microscope | Olympus | IX83 | |

XY(Z) Piezo System | Physik Instrumente | P-545.3R7 | |

100X Oil immersion objective | Olympus | UPLSAPO | |

QuadLine Beamsplitter | AHF Analysentechnik | F68-556T | |

Cobolt Jive 150 laser | Cobolt | 0561-04-01-0150-300 | |

Multimode Fiber | Thorlabs | UM22-600 | |

iXON Ultra 897 EMCCD camera | Andor | DU-897U-CS0-BV | |

Laser goniometer | SLS Systemtechnik | Mark III | |

CF40 Cryo-compact circulator | Julabo | 9400340 | |

Laser goniometer system | ALV GmbH | ALV / CGS-8F | |

Multi-tau corretator | ALV GmbH | ALV-7004 | |

Light scattering electronics | ALV GmbH | ALV / LSE 5004 | |

Photon counting module | PerkinElmer | SPCM-CD2969 | 2 units in pseudo cross-correlation mode |

633 nm HeNe Laser | JDS Uniphase | 1145P | |

F32 Refrigerated/heating circulator | Julabo | 9312632 |

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